4022_AppV APPENDIX V: FISH POPULATIONS

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APPENDIX V

FISH POPULATIONS

Appendix V.1 Photograph of Fish Sampling Locations

Photographs - Study Lakes

Photograph V.1 Consecon Lake (reference lake for white sucker), Moira River System, Fall 1999.

Photograph V.2 Round Lake (reference lake for white sucker), Moira River System, Fall 1999.

Photograph V.3 Moira Lake (exposed lake for white sucker), Moira River System, Fall 1999.

Photograph V.4 Stoco Lake (exposed site for white sucker), Moira River System, Spring 1999.

Photograph V.5 Bend Bay (exposed river site for white sucker), Moira River System, Fall 1999.

Photographs - River Study Sites

Photograph V.6 Site F-1 (reference site for longnose sucker), Moira River System, Fall 1999(view faces upstream).

Photograph V.7 Site F-2 (reference site for longnose dace), Moira River System, Fall 1999(view faces downstream).

Photograph V.8 Site F-3 (exposure site for longnose dace), Moira River System, Fall 1999(view faces upstream).

Appendix V.2 Golder Technical Procedure 8.1-3 Fish Inventory Methods

1 PURPOSE
2 APPLICABILITY
3 DEFINITIONS AND METHODS
REFERENCES AND SUGGESTED READING
DISCUSSION

LIST OF APPENDICES

Appendix I Maturity Codes and Definitions

1 PURPOSE

This technical procedure presents the techniques and methodologies used for standard fisheries sampling during fish inventory studies for the purposes of determining species presence, distribution, relative abundance, basic population characteristics and for conducting population estimates. Decisions regarding the type of sampling gear to use, the specific techniques to be employed and the timing of sampling will be determined prior to the commencement of the field study by the project team or project manager. However, due to the nature of fisheries work, some decisions regarding sampling specifics will depend upon conditions in the field. The methods for general fisheries inventory work are covered in this technical procedure. Other technical procedures are required in addition to this one in order to conduct fish sampling for specific tasks such as biomarking/fish health studies. This technical procedure does not detail the Quality Assurance/Quality Control requirements for components of field programs, such as note taking/data recording, as they are included in other documents.

2 APPLICABILITY

This technical procedure is applicable to all personnel involved in fisheries surveys for lakes and streams, including all sizes and orders of streams. It covers sampling equipment and techniques currently owned/used by Golder. Additional techniques are available which may be the most suitable method for specific circumstances or project requirements. If this is the case, the project manager must authorize the use of any new technique or the purchase of additional equipment.

3 DEFINITIONS AND METHODS

3.1 Abundance, Relative

The proportional representation of a species in a sample or a community. In fisheries inventories, relative abundance is typically used to describe the relative number of fish captured for each different species at a sampling site. Relative abundance can also be determined for the same species at different sites or in different seasons. It can also be determined for different life stages of the same species.

In some limited cases, the number of fish captured can be used to describe relative abundance. This is suitable for single effort in a single sampling area where relative abundance is simply the relative number of fish captured. For example, if 20 fish of one species and 10 fish of another species were captured in 100 seconds of electrofishshing at a site, species one is determined to have a relative abundance twice that of species two.

For any sampling situation which is more complicated, Catch-Per-Unit-Effort (CPUE) values must be calculated to determine relative abundance. CPUE values take into account the sampling effort required to catch the fish as well as the number of fish captured. For example, if 20 fish of one species were captured in 100 seconds of electrofishing at one site, and 20 fish of the same species were captured in 200 seconds of electrofishing at a second site, CPUE data shows that this species has a relative abundance at the first site which is twice that of the second site. In this example, twice the effort was required to capture the same number of fish at site two. This example also shows why it would be unsuitable to derive conclusions about relative abundance based solely on the numbers of fish captured.

In order to be able to determine relative abundance, you must record all sampling efforts in manner suitable for calculating CPUE data.

3.2 Ageing Structures

Ageing structures are bony parts of the fish which are taken for ageing analyses. In fish from temperate zones, these structures contain annual bands (annuli) which delineate seasonal variation in growth which can be counted to determine the fishes' age. Primary examples of these structures are scales, fin rays, saggital otoliths, cleithra and opercula. The appropriate ageing structures to collect vary according to fish species and life stage and include lethal and non-lethal sampling measures. Consult the table of "Recommended Fish Ageing Structures" (available in the aquatics reference file) for the appropriate structure and collection method for each species. With respect to fish ageing, all procedures used by Golder (i.e., the ageing structures which are collected and the methods used to determine age) conform to the manual of Fish Ageing Methods for Alberta (Mackay et al. 1990).

Following removal from the fish, ageing structures should then be placed in a "scale envelope", which consists of a small envelope which has been stamped with fields for recording the following information:

date
fish number
species
fork length
weight
life history stage
sex
state-of-maturity
sampling gear
sampling location
ageing structure collected
project number

Blank envelopes are ordered in bathes of 1000 and must be stamped prior to use. If your project includes the collection of ageing structures, it may be necessary to order the required envelopes and stamp them before heading out into the field.

The scale envelopes should be allowed to dry overnight before being stored. Upon returning from the field, the envelopes should be stored frozen in a one of Golder's freezers.

3.3 Anaesthetic

An anaesthetic is used in situations requiring live fish to be removed from the water and handled for extended periods, such as during surgery to implant radio transmitters, or to quiet fish for measurements. The anaesthetic commonly used by Golder is MS-222, known as tricaine methanesulfonate. The concentration of anaesthetic to be used depends on the required level of sedation. For surgery, which requires the fish to remain sedated for a period of 5-10 minutes, a concentration of 100 mg/L is used (i.e. 4g of MS-222 in 40 L of water). The fish is placed in the anaesthetic bath for 2-4 minutes until the desired level of sedation is reached. Care must be taken as overdoses lead to direct mortality. When monitoring the fish in the anaesthetic solution, watch for loss of coordination (when the fish no longer keeps itself upright) and respiration rate. Towards the end of the anaesthetization period, the fish will begin to "Cough".

Use of anaesthetic for quieting fish for measurements is not typically recommended unless the fish is difficult to handle or may injure itself. Fish anaesthetized with MS-222 are not recommended for consumption by anglers for a period of 2-4 weeks following exposure to the anaesthetic. Therefore, use only on fish which will not be captured and consumed or with permission of Alberta Fisheries Management Division.

3.4 Biomass

Biomass is the total mass (weight) of fish, or of fish of a given species, within a study area. It is a component of population estimates, as an estimate of the total number of fish in the study area is required to calculate biomass. Using either total removal data or a mark/recapture population estimate for the study site, the total biomass is calculated by multiplying the total population of fish by the average weight of the fish captured. Results can be expressed as units of weight over study area dimensions (e.g.kg/m of stream, kg/m² of lake).

3.5 Capture/Sampling Techniques

The following sampling techniques are used to capture fish. Some techniques are very specific to one life stage while others are more general. All sampling techniques have some degree of sampling bias associated with them with respect to fish size selectivity and sampling efficiencies based on environmental parameters such as water depth, conductivity, stream size etc. It is important to understand these biases when designing or implementing a study plan and when interpreting the data and drawing conclusions form the results.

3.5.1 Airlifting

Airlift sampling is used to collect fish eggs from the substrate for species which are broadcats spawners (i.e. do not bury their eggs). It can be used simply to determine if incubating eggs are present or to determine the relative density of eggs at each spawning site. The airlift sampler consists of a gas powered generator and compressor unit, a length of hose, an airlift head and couplers to connect the hose to the compressor and airlift head. The airlift head is attached to a long pole and consists of a 4" or 6" diameter hollow tube with a 90° bend at the upper end. The lower end of the airlift head has an internal tube which runs around the internal circumference and which is perforated. With the lower end of the airlift head held against the substrate, air is pumped from the compressor through a hose and into the perforated tube. Air rising inside the airlift head creates a vacuum effect which lifts loose particles up from the substrate. A removable collection bag placed over the upper end of the airlift head collects the particles. The sample is dumped into a sampling tray and examined for the presence of eggs.

This technique is employed when sampling water too deep to kick sample or when a quantitative sample is required. Since the area (cm²) of the airlift head is known, simply count the number of times the head is touched to the substrate for each sample in order to determine the number of eggs/cm² in the sample. Quantitative sampling can be used to determine the relative use of the spawning areas sampled, as determined by egg density. Remember to record the size of the airlift head used.

3.5.2 Angling

Angling refers to the use of angling gear, such as rod and reel, to sample for fish. Angling is an active technique using lures, bait or flies. Leaving a static, baited line in one place is referred to as a Set Line and is not an angling technique. On the other hand, jigging with a baited line would be an angling technique.

Sampling effort should be recorded as both the number of hours angled and the number of angling tools used. It would be recorded as angler-hours, or as rod-hours or some equivalent if more than one piece of angling gear is used per angler. The types of hooks, size of hooks, and number of hooks should also be recorded. In addition, notes on the types of habitats fished and the length of shore line covered if trolling is conducted should be recorded.

3.5.3 Drift Net

Drift net is a passive sampling technique for use in flowing water for the capture of life stages which are moving or drifting downstream. A drift net consists of a long, tapering net with an open mouth at the upstream end and a detachable sample sample bottle at the downstream end. Drift nets are anchored in place in the stream and filter the water passing through them, collecting materials from the water column. They can be placed to sample the bottom, middle or top of the water column or can be stacked to sample the entire water column. At regular intervals, the nets are removed and cleaned by dumping the collection jars into a sampling tray and examining the sample for the presence of fish. Typically the drift nets are checked and cleaned twice per day, once first thing in the morning and once again in the evening. Record the catch separately for each period to determine diurnal patterns.

Sampling effort is usually recorded as the number of hours between net cleanings to determine catch/hour. If more detail is required, it is also possible to estimate the volume of water sampled by the net during the period between net cleanings to determine the catch/m³. To do this, measure the velocity of the water at the sampling site before setting the drift net and again after lifting the net for cleaning to determine the average water velocity through the net Multiply the average velocity (m/s) by the area of the net mouth (m²) to get the volume sampled per unit time (m³/s) (remember to record the size of the drift net mouth). Multiply this value by the time the net was in place to calculate the total volume sampled. For this calculation, the drift net mouth must be completed submerged.

3.5.4 Electrofishing

Electrofishing refers to the use of electricity to stun and capture fish. An electrical current is passed between electrodes placed in the water and the resulting electrical field attracts passing fish (galvanotaxis) toward the positive electrode (anode). As fish pass close to the anode they encounter an increasingly stronger current gradient which acts as a narcotic and stuns the fish (galvanonarcosis), allowing them to be easily dip-netted from the water. Once captured, the fish may be identified, weighed, measured, tagged and then returned to the water. Fish taken by electrofishing revive quickly when returned to the water. Effort is automatically recorded by the electrofishing unit as the number of seconds of active electrofishing (i.e. the time current is applied to the water). Record the effort (seconds) immediately after completion of sampling and reset the timer to zero. Electrofishing techniques require experienced operators in order to reduce injury to the fish and to eliminate potential injury to the personnel involved. Safety training or working with experienced personnel is required for operating electrofishing equipment.

Backpack Electrofishing

Backpack electrofishing is a sampling technique for small, wadable streams. A backpack electrofisher consists of a portable electrofishing unit and a power source (12v battery or mini generator) attached to a pack frame. It is equipped with a hand held, button-operated anode pole and a cathode plate which is left trailing in the water. the operator wears the pack unit and used the button switch to activate the anode in order to stun fish while wading instream. One or more assistants wading next to the operator use dip nets to capture the stunned fish. The assistant also adjusts the electrofisher settings for the operator and monitors the electrical output. Sampling is normally conducted while moving upstream so that fish are not disturbed, prior to being sampled, by disturbances to the stream bed and material moving downstream with the flow.

Boat Electrofishing

Boat electrofishing is an extremely effective sampling technique for moderately shallow water and is used for intermediate streams, large rivers and shallow littoral areas in lakes. Two types of boat electrofisher are available, both of which consist of an electrofishing control box which is powered by a 5,000 watt generator. The portable boat electrofisher has a free control box and generator which can be loaded into an inflatable boat (Zodiac) and is ideal for small or intermediate sized rivers which cannot be waded and which cannot be effectively sampled by the low current outputs provided by a backpack electrofisher. Two anodo configurations are possible, depending on stream size, and include either a hand-held, button operated anode pole or a foot-switch operated portable boom system. In both cases, a floating cathode plate is employed. The boat can be drifted downstream or an outboard jet can be used to provide increased mobility. In comparison, an electrofishing boat consist of an 18' aluminum river boat with an integral electrofisher control box and generator. It is also equipped with a work platform and flow-through live well for holding fish. It has a foot-switch operated anode boom system and uses the boat hull as the cathode. Boat electrofishers are designed for any intermediate or large river which is deep enough to allow a boat of this size to float and which has a site with a suitable boat launch. This unit has the largest abode/cathode surface area and is capable of generating the largest electrical field and the highest current outputs. Boat electrofishing sampling for both type of units is usually conducted while floating downstream, as this makes fish easier to dipnet and puts less stress on the dipnets and anodes.

3.5.5 Emergent Trap

An emergent trap is a passive sampling technique specifically designed to capture fry as they emerge from the substrate following hatching. A typical emergent trap consists of a square metal frame (0.3m x 0.3m) covered with a small mesh net and collection bottle. The mouth of the trap is placed on top of the substrate at a known or suspected spawning area where incubating eggs are known or thought to be present. It is left in place through the incubations period. Once the fry have hatched and absorbed their yolk sacs they emerge from the substrate. The fry from the eggs which were located under the trap mouth will be captured by the trap.

Emergent traps can be used to verify a suspected spawning area or to check for hatching success at a know spawning site.

3.5.6 Fry Traps

A fry trap is a passive sampling technique used to capture fry which are drifting downstream in flowing water. It is suitable for capturing fry which are larger than post-emergent size but which are not yet strong swimmers. The fry trap is anchored to the stream bed using 2 rebar posts and consists of a large metal frame open at the upstream end and otherwise covered with small mesh metal screening. "Wings" lead from the trap mouth into a low velocity area at the downstream end of the trap where the fry accumulate. The trap is designed so that it will pivot at the anchor point on the stream bed. To check the trap, simply tilt it forward and hold a collection bucket in front of the "top" of the low velocity holding cell. Water and fry from the holding cell will pour into the bucket as the trap is tilted. Typically the traps are checked and cleaned twice per day, once first thing in the morning and once again in the evening. Record the catch separately for each period in order to be able to determine diurnal patterns.

Sampling effort is usually recorded as the number of hours between trap cleanings to determine catch/hour. If more detail is required, it is also possible to estimate the volume of water sampled by the trap during the period between trap cleanings to determine the catch/m³. To do this, measure the depth and velocity of the water at the sampling site before setting the trap during the sampling period. Multiply the average depth (m) by the average velocity (m/s), then by the width of the trap mouth (m) to get the volume sampled per unit time (m³/s) (remember to record the width of the trap mouth). Multiply this value by the time the trap was in place to calculate the total volume sampled.

3.5.7 Gill Netting

A method of capturing fish that involves the setting of nets of various mesh sizes anchored in place in a river or lake. A gill net consists of netting suspended between a weighted "lead" line and buoyant "float" line which, when set, forms a vertical wall of netting. The lead line is attached at both ends to heavy weights to hold it in place and keep the net taught. The float line is attached at either end to floats. In Alberta, the floats must each consist of a pole which stands upright at the water surface and extends above the water surface for a minimum of 1.0 m. The top of the poles must have a blaze red or orange flag measuring at least 20 cm x 20 cm and market with the Fish Collection Licence Number in 20 mm high letters. Typically, we use sandbags filled with rocks or sand from the gill net site for lead line weights. This way, all we have to carry with us to the site is a few empty sandbags. New gill nets need to have a length of sideline attached to either end which extends from the float line to the lead line to take the tension when the net is lifted to ensure that the mesh does not rip.

Gill nets are designed to function by catching on the gill covers of fish as they attempt to swim through. Fish of a size for which the gill net mesh size is designed swim into the net but can only pass partway through the mesh. When the fish struggles the twine slips behind the gill covers (opercula) and the fish becomes "gilled". Therefore, the mesh size of the gill net is important when selecting a net or nets for your sampling activity as gill netting can be a very size selective technique.

Gill net mesh size can be measured as either the stretch measure of square measure of the openings in the mesh. At Golder, we always use the stretch measure to identify our gill nets and when reporting results. The stretch measure is the distance between two opposite corners of the square mesh opening, when the square is stretched flat. Gill net mesh sizes typically range from 1.9 to 14.0 cm (3/4" -5.5"). As most gill nets are sold using imperial units of measure, the following table will help you convert mesh sizes to metric units.

Stretch Mesh Sizes:

Imperial (inches) 3/4 - 1.0 - 1.5 - 2.0 - 2.5 - 3.0 - 3.5 - 4.0 - 4.5 - 5.0 - 5.5

Metric (cm) 1.9 - 2.5 - 3.8 - 5.1 - 6.3 - 7.6 - 8.9 - 10.2 - 11.4 - 12.7 - 14.0

Gill net meshes are constructed either of monofilament or nylon. Monofilament is sturdier and longer lasting but gill nets made from this material do not compress and take up a much larger volume than a nylon net of the same dimensions. For longer nets, the volume of a monofilament net becomes significant.

Gill nets can be simple or multi-mesh. Simple nets consist of one mesh size only, although different nets may have different lengths and depths. Multi-mesh nets are also called "gang" nets and consist of more than one mesh size. Each mesh size occurs in a discreet section of the net which is called a panel. Gang nets typically have from two to five different mesh sizes or panels. Usually, each panel has the same length, although this is not always the case. An important component of recording sampling effort is to record the dimensions of all gill nets that are set. Record the depth of each net as well as the total length. Also record the number of panels, the mesh size of each panel and the length of each panel. Effort should also be recorded as the number of hours the net is set and CPUE is expressed as either duration (hrs), panel-hours, or meter-hours, depending on the type and variety of nets set.

Since the size of the mesh will have a major role in determining the size of fish (i.e.species or life stages) that will be captured, it is extremely important to record the mesh sizes of any gill net used. It is also important to record the catch for each individual panel or mesh size. The field form used to record the catch has a space for recording the mesh size for each fish captured. When removing fish from the gill net, the fish must be separated by mesh size.

Selecting a gill net or nets to be used for a project will vary depending on your sampling goals. Long gang nets with several different mesh sizes, from small to large mesh, are best for general inventory sampling and have the smallest level of sampling bias. For single mesh nets or nets with few panels, it is generally true that the larger the mesh size used the larger the fish that will be captured. The small 1.9cm mesh nets will capture fish as small as the larger minnow species and juvenile life stages of larger fish. Mesh sizes in the range of 5.1-7.6 cm are typically used for salmonid species while larger mesh sizes will be employed to capture adult northern pike and burbot. Most gill nets will capture a larger size range of fish than mesh size would dictate as some species will be captured without necessarily being "gilled". For example, suckers may be entangled by their large lips and northern pike often bite and roll in the mesh, becoming entangled in mesh sizes too small to capture them by gilling. Bullheads on the other hand are often captured in mesh sizes too large to gill them when their pectoral and dorsal spines become entangled in the mesh.

Nets selected for sampling in rivers are generally different from those used in lakes. River gill nets typically have large floats attached to the float line for added buoyancy. Shorter nets are used as they must be set in low velocity pockets such as backwaters or pools and heavy weights are used to anchor the net so that it will remain in position in flowing water. Caution should be taken when setting nets in a river at high stage if floating debris is moving downstream which could damage or move the net. In lakes, much longer nets can be used if required and, since lakes typically have greater depths than rivers, nets can be set at a variety of depths. Lake nets can be set so that they float near the surface, are set along the lake bed or are positioned in mid column. For floating sets, nets with large floats attached to the float line can be used and long leads are tied to the weights to allow the net to remain at the surface. For sinking sets, nets without additional floats or with small floats are used. For bottom sets, the weights are tied tight to the lead line and long leads are tied to the floats so that the net will sit on the bottom and the floats will remain at the surface. For mid column sets, leads are attached to both the weights and floats so the net will be positioned between the bottom and the surface.

Gill netting is a sampling technique that can be used in the winter as nets can be set under the ice. In lakes where there is no current a jigger is used to run a length of sideline under the ice. A large hole is opened in the ice and the jigger is placed under the ice. The sideline is tied to the jigger and the lever arm is manipulated to send the jigger moving away from the hole. Once the jigger has moved far enough it must be relocated, either by sight if the ice is clear or by sound as the jigger is equipped with a "clicker" device. A hole is drilled at the location of the jigger and a hook is used to pull the sideline up the hole. In rivers or in the case of thick lake ice a Murphy stick is used to set the net. A Murphy stick consists of two sections of aluminum pipe hinged together which extends as an under-ice probe. The far end of the probe has an eye-hook at the end and a float a short distance back. A length of sideline a little longer than the gill net is tied to the eye-hook and the far end of the probe is pushed down through one hole in the ice and manoeuvred towards a second hole where the attached sideline is hooked and pulled up through the hole. The process is repeated several times to extend the rope as far as desired. Once the sideline has been placed under the ice it is then attached to one end of the gill net and used to pull the net under the ice.

As a sampling technique, gill nets can have a high mortality rate if the fish are left in the net for a prolonged period or if water temperatures are high. If fish mortality is a concern, the nets should be cleaned of fish on a regular basis (e.g. every two hours). If mortality is desirable (i.e. fish are to be sacrificed) or not a concern, nets should be set overnight in order to sample day and night periods of fish movements and to allow capture of fish which may avoid the net if it is visible during daylight hours in low turbidity water.

3.5.8 Hoop Net (Fyke Net)

A hoop net is cylindrical net distended by a series of hoops or frames with one or more internal funnel-shaped throats whose tapered ends are directed inward from the mouth to prevent fish from escaping once they enter the net. A fyke net is a hoop net with tow wings or leads of webbing attached to the mouth to guide fish into the enclosure. Our hoop nets have large square hoops at the front of the net and taper to a smaller diameter with smaller ring hoops at the back end. Webbing extends inwards and backwards between the sides of the first square hoop to form a "V" slot at the net mouth and a funnel is attached to the back of the second square hoop. The chamber between the funnel and the rear of the net is termed the "pot". The net is tapered at the rear end and held closed with a draw string which can be opened to permit removal of the trapped fish from the pot, although trapped fish may also be present between the "V" slot and the funnel. The funnel also has a draw string which allows removal of fish from this chamber. If it is desirable to have a fyke net, use two lengths of webbing tied to the sides of the hoop net mouth to convert the hoop net to a fyke net.

Fyke nets are typically set at a time and location where fish will be moving through the area in a direction that will lead them into the net mouth. They are very effective when set in small tributaries to lakes or larger rivers during a spawning run but can also be used in shallow areas of lakes and larger rivers. The net and wings are anchored in place by tying them to rebar posts embedded in the substrate. The wings of the net should be set at a 45° to the axis of the hoop net.

As the holding chambers in the fyke nets are small, they should be checked and cleaned of fish on a regular basis, particularly during an active spawning run. Try to set the net so that fish in the holding chamber will not be subjected to high water velocities. Sampling effort is usually recorded as the number of hours between net cleanings. Record fyke net dimensions such as mesh size, mouth size, wing lengths and, when used in streams, whether full or partial channel blockage was achieved and whether the net mouth was oriented upstream or downstream.

3.5.9 Kick Sampling

Kick sampling is used to collect fish eggs from the substrate in spawning areas, both for species which are broadcast spawners and for those which fbury their eggs (i.e. from trout redds). It can be used to determine if incubating eggs are present but it is generally considered a qualitative (i.e. non-quantitative) sampling technique and, unlike airlifting, is not suitable for determining the relative density of eggs. The kick sampler is attached to a pole and consists of a tapered net attached to a metal frame which forms the mouth of the net. It is generally used in flowing water. To use, grasp the pole and place the kick net against the substrate. Stand upstream of the net mouth and use your feet to disturb the substrate, letting the disturbed materials float into the net. Remove the net form the water and examine the contents of the net for eggs.

Kick sampling can only be conducted in water shallow enough or which is flowing slow enough to allow instream wading. This technique is simpler to use than the airlift sampler and requires considerably less equipment. It is a very efficient and fast technique for identifying spawning areas in wadable streams, particularly over long lengths of stream.

3.5.10 Minnow Trap

Minnow trapping is a passive sampling technique used to sample for the presence of minnow species and small life stages (i.e. fry) of larger species which can be difficult to capture using other techniques such as electrofishing or gill netting. The traps we use are Gee Minnow Traps which consist of two pieces which are clipped together to form a small cylinder slightly tapered at either end. Each end has a funnel which leads into the centre of the trap which allows fish to enter but prevents them from escaping. The traps are generally placed on the substrate in the shallow shoreline areas of lakes and streams with the long axis of the trap parallel to the shoreline. A length of sideline is used to tie the trap to a stake or anchor on shore to keep it in place. The anchor site is usually flagged so that the site can be easily found when returning to check the trap. The traps can be baited or unbaited, depending on if the intent is to trap fish moving through the area or attract fish to the trap.

Sampling effort is recorded as the number of hours that the trap is set.

3.5.11 Observation

Underwater observation involves the use of either snorkeling or SCUBA techniques to observe, count or record the activities of fish. Scuba diving is generally restricted to lake habitats but may also be employed in deeper rivers. It is a fairly intrusive technique and is considered to be more disruptive than snorkeling and requires that the observer have a valid scuba certificate. Snorkeling is commonly employed by Golder to conduct fish observations in stream habitats which have low turbidities. It is less disruptive than SCUBA and logistically simpler. Equipment used for snorkeling includes a diving mask, snorkel, dry suit, diving gloves and an underwater writing slate. A wet suit can be used in place of a dry suit in warm water but a dry suit is preferable as it increases observation time. To date, snorkeling has been used by Golder to study the habitat preferences of some fish species but the technique can also be used to determine fish abundance and distribution.

3.5.12 Post-Emergent Trap

Post-emergent traps are a passive sampling technique for use in flowing water to sample for the presence of post-emergent fry. Unlike emergent traps which capture the fry as they emerge from the substrate, post-emergent traps capture the fry as they drift downstream following emergence. Unlike emergent traps, it is not required that they be set at a spawning site overtop of incubating eggs, there only needs to be a spawning area somewhere upstream of the set location. Post-emergent traps are essentially extremely large drift nets. Each trap consist of a tapered, small-mesh net attached to a metal frame which forms the trap mouth. The trap mouths are 0.9 x 0.9 m in size. Each et is equipped with a removable sample bottle attached at the downstream end of the net. A post-emergent trap is set by anchoring two rebar poles into the substrate and looping the four hoops attached to the trap over the poles and sliding the trap down until the bottom of the trap sits on top of the substrate with the mouth facing upstream.

Post-emergent traps should be checked at a minimum of twice per day, once in the morning and once in the evening Definite diurnal/nocturnal patterns have been observed using these traps, so be sure to record the catch separately for each sampling period. To check the catch, remove the trap from the stream and wash all materials from the netting into the sample bottle. Dump the contents of the bottle into a sampling tray to look for the fry. Post-emergent fry are extremely small and almost transparent. They are best seen by looking for the large, dark eyes which will be their most obvious feature. They may also be seen to be swimming around in the sampling tray. It is also prudent to check the mesh of the trap for additional fry as they are so small that some become "gilled" on the mesh and do not wash down into the collection bottle. If more than one species may be hatching at the time and location of your study and you are not sure of the identification of fry in the sample, the sample should be preserved in 5% buffered formalin for laboratory identification.

Sampling effort is recorded as either catch/hr or catch/m³, as described for fry traps (Section 3.5.6). Post-emergent traps are used to check for the presence of post-emergent fry in the study area, either as proof of spawning activity in upstream areas or simply to tell if this life stage or a certain species is present. They are also used in entrainment studies, which are conducted to determine if fish are entering man-made structures such as diversion canals or water intakes. In addition, they may be used to determine the timing of hatching periods and the relationship between hatching and environmental parameters such as discharge or water temperature.

3.5.13 Seine Netting

Seine netting refers to the use of a specifically designed net to catch fish by dragging it through the water. Seine nets consist of netting suspended between a float line and a lead line. The netting is constructed of ticker net material than gill nets so that fish do not become gilled in the mesh. Mesh sizes vary but most nets are constructed of minnow netting which has a small mesh size and is suitable for catching forage fish and small life stages of larger fish species. Larger mesh seine nets are also available for sampling for large fish and are much easier to drag through the water. Two types of seining operations are possible, beach seining and boat seining.

Beach seining is accomplished by two people dragging the net through the water while wading and is used in shallow water areas in lakes and streams. To beach seine, each person grabs one end of the net by placing one foot in the loop at the end of the lead line and holding the loop at the end of the float line in their hands. One person walks out from shore to a suitable depth. Both people then walk parallel to shore dragging the net between them. The lead line is kept in contact with the substrate to prevent fish from escaping under the net by dragging the foot looped to the lead line along the bottom. As they walk through the water, fish are herded in front of the net. The person near shore moves slower than the person further out. When the further person has passed the near shore person they curve back to shore, meeting the near shore person at the waters edge and bringing the two ends of the net together forming a pen holding the captured fish. Both people then drop the float lines and pick up the leads lines and standing side-by-side pull the net up on shore, ensuring that the lead line remains in contact with the substrate at all times. The trapped fish will congregate in the end of the looped net and will be dragged up onto shore.

Boat seining is a specialized technique used in water too deep to wade. It usually involves the use of long, large mesh seine nets for the capture of large fish. It is particularly useful in areas where fish congregate such as spawning areas of lakes or snye areas in rivers. The principle is similar to beach seining except that a boat is used to move the offshore end of the net through the water. A pole is attached to both the lead and float lines, at the boat end of the net, and is used to keep the lead line on the bottom.

Seine netting is a suitable technique only where the bottom is fairly smooth. If large substrate particles, debris, or aquatic vegetation is present which will cause the lead line to lift off the bottom as it passes, the technique will not be very efficient and most or all fish will escape. Seine netting is typically used to sample for the presence and abundance of small fish and life stages which are not effectively sampled for using other inventory techniques.

Sampling effort is recorded as the number of seine hauls made and either the distance (m) or the area (m²) seined for each haul. Record the dimensions of the seine net used (length/depth/mesh size) and the shoreline distance of each seine haul. If area is required, multiply the length of the seine haul by the length of the seine net used.

3.5.14 Set (Trot) Line

A set line is a series of leaders and baited hooks strung from one central line which is anchored to shore. Set lines are used to catch predatory fish and are usually set out overnight. Golder set lines are 30 m in length, which includes a 10 m lead with no hooks and 20 m of line with a total of 10 leaders/hooks set at 2 m intervals. A large lead weight is attached to the end of the line to keep it in place once it is set. The 10 m lead is used to set the baited hooks well out from shore or can be tied short to keep the hooks near shore, as desired.

Sampling effort is recorded as the number of hours the line is set or the number of hook-hours if set lines of different lengths and number of hooks are used. Record the size of the hooks that are used (e.g. #8 hooks).

3.5.15 Trap/Counting Fence

Fish traps or counting fences are a passive sampling technique used to capture fish as they move past a specific location. They consist of one or more trap boxes with fences (wings) which stretch out in front of the entrances of the boxes to lead fish into the trap. The trap boxes are large holding pens enclosed on four sides as well as on the bottom with metal or plastic mesh. The front of each box has an opening equipped with a funnel which leads into the interior of the trap box. The fences consist of angular aluminum frames with a series of holes into which are fitted round aluminum rods to form a barrier to fish passage. The counting fence is installed by attaching the components to rebar posts driven into the stream bed and by placing sandbags on cradles included in the fence design. The fences or wings are set as close as possible on a 45° angle to the trap box entrance.

Two types of counting fence set-up are possible, the one-way fence and the two-way fence. The one-way fence has only one trap box and one set of wings and is used to capture fish moving in one direction. The two way fence has two trap boxes facing in opposite directions, each with its own set of wings, to capture fish moving in both directions. Counting fences can be used to sample portions of the shoreline in lakes or large rivers but are typically used in small or medium sized streams to close off the entire channel and capture all fish moving past the trap location. In this case, the box which captures fish moving upstream is called the upstream trap and the box catching fish moving downstream is called the downstream trap. In streams, the trap boxes should be set in a location where the water velocity is not too high so that the fish caught in the trap can rest. If no such site is available, a piece of plywood placed upstream of the trap will provide a velocity shelter

The counting fence should be checked a minimum of twice a day, once first thing in the morning and once again in the evening and the fish removed from the traps using a dipnet. The fence should also be cleaned of debris to keep the water flowing freely through it and to reduce the build up of pressure on the fence. Record the day, time and catch each time the fence is checked. During an active spawning run, the fence may need to be checked more frequently so that the number of fish holding in the trap boxes does not become too large. Record the catch separately for each sampling period. After removing the fish from the trap boxes they should be released in the direction that they were travelling so that they can continue in that direction (i.e. fish from the upstream trap should be released upstream of the counting fence while fish from the downstream trap should be released downstream of the fence).

Counting fences are used to determine the species, relative abundances and timing of movements of fish past the sampling site. They are typically used to capture fish during their spawning runs in the spring or fall or to quantify the movements of fish into and/or out of tributary streams.

3.6 Catch-Per-Unit-Effort (CPUE)

Catch-Per-Unit-Effort is a measure which relates the catch of fish, with a particular type of gear, to the sampling effort expended; it is expressed as: number of fish captured/unit of effort. Results can be given for a particular species or the entire catch. CPUE is used to define species relative abundance and to compare abundances between sites and/or seasons. Effort can be expressed a number of ways depending on the sampling equipment. If CPUE data is required, sampling effort must be recorded. Following are common CPUE calculations for traditional sampling gear:

• electrofishing (boat and backpack)	No. of fish/100 seconds (of active electrofishing)
• gill net	No. of fish/net-hour, or/panel-hour, or/100m of net-hour
• set line (trot line)	No. of fish/hour, or/hook-hour
• angling	No. of fish/hour, or/angler-hour, or/rod-hour
• minnow trap	No. of fish/hour, or/trap-hour
• seining	No. of fish/area seined (m²), or/length of shoreline seined (m)
• counting fence (fish trap)	No. of fish/hour, or/hour
• drift net/post-emergent trap	No. of fish/hour, or/volume of water (m³)

It is important to recognize the components of the effort inherent in the sampling technique being employed so that effort will be recorded properly. Most field forms will have fields specifically designed to record the pertinent information. Record all aspects of your sampling effort (e.g., number of set lines used and number of hooks perline) so that CPUE can be calculated. CPUE values will be used in our own studies to establish relative abundance. Our data may also be used in a more historical context to compare the abundances we record with past or future research, using both similar and different sampling gear, and CPUE values may need to be recalculated to conform to other studies. The more detailed used when recording sampling effort, the easier it will be to accommodate these needs.

3.7 Coldwater Fish

When dealing with the general suitabilities of freshwater habitats for game fish species, temperature regime is often used to describe the habitat potential and the species assemblage which could possibly be present. Although the terms are not definitive or precise, the designations of habitats as "coldwater" or "coolwater" habitats and the associated fish fauna as "coldwater" or "coolwater" species are often used.

Coldwater fish are those which have a preference for summer water temperatures ranging from about 10-18 °C. In Alberta, this ecompasses all of the salmonid species including the trouts, whitefishes and Arctic Grayling. Within this group the species will have differing temperature preferences and tolerances (see section 3.50 - Temperature Criteria).

3.8 Condition Factor (Ponderal Index)

Condition factors are used to describe the plumpness and, by inference, the well-being of individual fish. Formulas are used to calculate condition factors using the fish's length and weight and are based on the principle that the weight of a fish will vary with the cube of its length. Any variation in the shape or plumpness will be measured using the formula. Golder primarily uses the coefficient of condition K, also called the Fulton condition factor. The formula (using metric length and weight data) is as follows:

K=[weight (g) x 10⁵] / fork length³ (mm)

Condition factor is believed to reflect the nutritional state or well-being of an individual fish. The K value will be 1.0 for fish whose weight is equal to the cube of its length. Fish which have a K value >1.0 are more plump and are thought to have a higher degree of well-being or better nutritional state-of-health, whereas fish with a value <1.0 are considered to be less robust.

Condition factors vary with season, sex, sexual maturity, age and various other factors. Therefore, if sufficient data is available, average condition factors for a species should be calculated separately for each sex and should exclude young-of-the-year fish. Condition factors also vary by species, particularly if they have different shapes, and should not be used to compare well-being between fish species. They can, however, be used to determine differences in the condition of fish of the same species in different years or at different sites. Fulton's condition factor is also limited for comparisons between fish populations in different lakes because of differences in growth parameters. Other formulas for condition factor calculations are available and would be designated by the project manager if they are required.

3.9 Coolwater Fish

Coolwater fish are those which generally prefer summer water temperatures ranging from about 18-26°C. Alberta species generally considered to belong to this group include northern pike, walleye, sauger, yellow perch, goldeye, mooneye and lake sturgeon (see also Section 3.7-Coldwater Fish).

3.10 Creel Census

The term "creel" refers to the basket a fisherman uses to hold the fish which have been angled and a creel census refers to a survey in which recreational fisherman are censused in order to determine aspects of the recreational fishery. Important survey goals typically include determining angler effort and success (i.e. fishing pressure and harvest) and may include examining the fisherman's catch for tagged fish or to collect ageing structures.

3.11 Dissolved Oxygen Criteria

The dissolved oxygen concentration in the water is an important habitat component. Different fish species have different dissolved oxygen requirements and have different tolerances to low dissolved oxygen levels. Dissolved oxygen criteria provide minimum dissolved oxygen levels that are necessary to protect various life stages and have been developed for selected game fish species. Golder has prepared a document which list the criteria for selected Alberta species (Taylor and Barton 1992).

3.12 Fecundity

The most common measure of reproductive potential in fish. Female reproductive potential is the total number of eggs (ova) in both ovaries of a gravid female fish. Fecundity normally increases with the size of the female within a given species. For most studies conducted by Golder, fecundity is determined for female fish only. Fecundity is determined by recording the total weight (g) of both ovaries and removing a small sub-sample of known weight from the middle of the ovaries (usually a 1.0 g sample). Count the number of eggs in the sub-sample to determine the number of eggs/g of ovary. Multiply this value by the total ovary weight to calculate the total number of eggs.

3.13 Field Forms

Golder uses a number of specially designed field forms to aid in recording field data. They are not meant to replace the use of a field book or the recording of detailed field notes. They are intended a provide a template showing the type of supporting data that must be recorded for each sampling technique and provide an organized method of recording the sampling results. For each specific or general type of sampling technique there is a Catch Record Form (e.g. Gill Net Catch Record Form) for recording sampling information such as location, technique, effort and is used to summarize the results. The main form for recording the catch results is the Fish Sample Record Form which has fields for recording length and weight data and other particulars for each individual fish. On the back of this form you will find a list of all abbreviations to be used when recording data.

A copy of each field form is kept in the aquatics reference file located at Carole Collins desk (Aquatic Ecology Group Secretary). Copy the forms you will require onto waterproof paper and return the originals to the file.

3.14 Fish Collection Licence

Fish collection licences or permits are granted by provincial governments or by DFO and are required for all fisheries sampling activities. Obtaining a license varies from province to province. In Alberta, a Fish Collection Licence is granted to Golder by Alberta Environmental Protection, Fisheries Management Division. Each Licence is specific to the waterbody(s) being sampled and is valid for a specified tiem period. To obtain a Licence you must forward a letter of request to the F & W District office for the region in which you wish to sample. Include in the letter the reason for sampling, the location(s) to be sampled, the period the permit should be valid for, the capture techniques to be employed, the fate of the fish captured (i.e. will any be sacrificed), and the personnel to conduct the sampling. They will then send a Licence granting permission to carried out the proposed activities. They may impose specific restrictions on the licence (i.e., restricted number of fish allowed to be sacrificed, designation of a certain landfill for fish disposal, or specific reporting requirements) and the permits should be read carefully to ensure all restrictions will be followed. The original permit or licence should be immediately placed in the project file and a copy of the document given to the field personnel. You must be prepared to produce a copy of the permit while conducting any field sampling.

The Fish Collection Licence will also specify a date by which a permit return is to be submitted to the issuer. In Alberta, the permit return is a form which accompanies the Licence. The form requests information regarding the sampling conducted under authority of the Licence, such as sampling locations and results. Fill out the form and send it to the office which issued the Collection Permit following completion of sampling activities and prior to the date specified on the Licence.

3.15 Forage Fish

A general term applied to smaller species of fish that "forage" on small invertebrate animals or plant materials. This includes minnow species and other small fish such as sculpins, stickleback, trout-perch and darters.

3.16 Game (Sport) Fish

Fish used by anglers for recreational fishing or sought after by the commercial fishing industry, e.g., northern pike, walleye, trout, etc.

3.17 Geographical Position

All sampling sites, whether they are point locations (such as a minnow trap site) or sections (such as a section of river that was electrofished), should be recorded on a map of the study area. The standard is to use a 1:50,000 NTS topographical map but other maps or airphotos can be used if they provide greater detail. The geographical position of sampling sites can also be recorded using Universal Transverse Mercator (UTM) grid coordinates or by degrees of latitude/longitude. UTM coordinates are particularly useful in case the map is lost as they can be used to pinpoint the sampling site on a new map.

UTM and latitude/longitude are two different systems of grid coordinates used to establish geographical location. Both systems appear in the margins of 1:50,000 scale National Topographical Service maps. A calibrated ruler is used to calculate coordinates of any point on the mapsheet. Golder always uses UTM coordinates rather than lat/long, unless otherwise specified by the client.

The most accurate way to record the position of the sampling site is to use Geographical Position System (GPS) technology. If possible, use a GPS rover unit to record a position file at the sampling site that can be stored for differential correction. You should also use the GPS unit to record a "real-time" waypoint in the event that the stored file is lost or accidentally deleted. If you do not have a GPS unit capable of differential correction, a simpler unit will allow you to record a waypoint, which will be less accurate.

3.18 Gradient

Gradient refers to the vertical drop in elevation along a watercourse over a horizontal distance. It is recorded as the percent gradient. To determine the gradient over a length of stream, measurements are taken off of a 1:50,000 scale NTS map of the watercourse. Locate a point upstream and downstream of the study area on the map where contour lines cross the stream and determine the difference in elevation (m) between these two points. Measure the distance (m), following the channel, between the same two points using a map wheel. The gradient is calculated as follows:

gradient (%) = [difference in elevation (m)/distance (m)] x 100

In very flat terrain determining gradient from a map may not be possible. In these situations, gradient may also be measured in the field using a clinometer. With this method one person with a clinometer stands at the upstream end of the section to be measured, a second person moves as far downstream as possible while still visible to the upstream person. Both individuals stand at the very edge of the stream with their feet at the water surface. The upstream person uses the clinometer to measure the angle from his or her eyes to the eyes of the other person. If your clinometer measures in % then this value should be recorded. If the clinometer measures in degrees, then percent can be calculated by taking the tangent of that number and multiplying by 100. This technique may need to be repeated several times and averaged to determine the gradient of a large section of stream.

3.19 Growth

Fish show indeterminate growth in that they continue to grow throughout their lives rather than stop growing once they reach an "adult size". However, growth rate is asymptotic, meaning the growth rate decreases with increasing age approaching some maximum value for the individual or population. As growth rate is a function of time, true growth rates can only be determined when fish length and age is known. Two parameters related to growth rate are: 1) the maximum size which is possible for fish in a given population, and; 2) the rate at which maximum size is achieved. The maximum size value indicates whether the population is "stunted" (i.e. does not have the potential to reach the normal maximum size for the species) and differentiates between populations that are stunted and those which do not achieve their potential maximum due to a short life span. If the maximum size for the population is at the lower end of the normal range for the species. than the population is slow growing rather than stunted. See Mackay et al. (1990) for methods of calculating maximum size and rate.

3.20 Gonads

Organs which are responsible for producing haploid reproductive cells in multicellular animals. In the male, these are the testes and in the female, the ovaries. In fish they are located in the peritoneal cavity, extending between the disphragm and the cloaca, and running along the dorsal side of the cavity along both sides of the spine. When the fish is gravid, the gonads will fill much of the peritoneal cavity.

3.21 GSI (Gonadal:Somatic Index)

Gonad-Somatic Index is the proportion of reproductive tissue in the body of a fish to total body weight. It is calculated by dividing the total weight (g) of the gonads by the total body weight (before gonad removal) and multiplying the result by 100. It is used as an index of the proportion of growth allocated to reproductive tissues in relation to somatic growth. It is believed to be an indicator of fish health in that a fish with a comparatively low GSI for its species is considered to not have sufficient energy available for proper gonad growth. Fish are seasonal spawners and the size of the gonads changes dramatically as they pass through the various stages of gamete maturation. It is preferable to conduct GSI measurements for fish just prior to the spawning season when the gonads are fully developed (i.e. gravid).

3.22 Habitat

Fish habitat refers to aspects of the physical environment which provide the requirements of a fish community, species or life stage. Habitat evaluations conducted for fisheries studies generally involve measurements or evaluations of macro-and/or micro-habitat conditions in order to determine the types of fish or life stages an area might support, the quality of available habitats or habitat limitations.

Macro-habitat

Macro-habitat refers to habitat components which are attributable to a general region or section of the study area. They are general conditions related to geographical location, climate, stream order, lake type, etc. For macro-habitat evaluations, we typically measure general water quality parameters (dissolved oxygen, temperature regime, pH, conductivity, turbidity, visibility (secchi depth), stream gradient), as they relate to describing coldwater and coolwater habitats and the types of fish species which may be present. Different fish species have different tolerances for macro-habitat conditions which affect their abundances and distribution.

Micro-habitat

Micro-habitat conditions are the physical conditions at a specific location. For micro-habitat assessments we measure or evaluate water depth, velocity, substrate particle size and condition, and the availability of cover for fish. Cover includes instream cover (i.e. any objects which provide velocity shelters) and overhead cover (i.e. anything which provides visual isolation). Each fish species has a range of micro-habitat conditions which are suitable, ranging from barely useable to optimal. In addition, each species has a series of life stages which may also have different habitat requirements. These life stages include spawning, incubation/embryo, nursery, rearing, feeding (adult summer) and overwintering.

Knowledge of the suitable and preferred habitat conditions for different species and life stages is very useful when conducting fisheries inventories, habitat evaluations and impact assessments. Information concerning these habitat requirements is available in the form of Habitat Suitability Index (HSI) models and Habitat Preference Criteria (HPC). HSI modesl were developed by the U.S. Fish and Wildlife Service and are species-specific modesl, with each model containing information for all life stages of one fish species. The models include all the habitat variables (macro-and micro-habitat) that accumulated research has determined to be significant to each species with respect to population abundance. Each habitat variable is provided along with the range of suitable and optimal conditions. HPC are species-specific curves showing suitable and preferred conditions for micro-habitat variables (depth, velocity, substrate and cover). HPC curves are available for a limited number of game fish species and were developed from snorkeling observations of the different species and life stages (developed for the most part by Golder from streams in Alberta).

Measurements of macro-and micro-habitat conditions in lakes and streams are useful in combination with inventory data and existing information to establish habitat potential for a study area. Habitat based assessments are being used more frequently to provide a complete picture of habitat potential, with respect to use by different fish species and life stages, rather than relying on fish inventory data from a specific point in time.

3.23 Length

Refers to the whole body length of a fish. There are three types of length measurements: standard length, fork length, and total length. The measurement most commonly used in Canada and required for use by Golder is the Fork Length and is always recorded in millimetres (mm). Fork length is the distance from the most anterior point on the head to the tip of the median caudal fin rays. The fork length of captured fish is measured on a fork length board, which is a trough or flat board with a ruler attached to the surface and a vertical block at the anterior board, which is a trough or flat board with a ruler attached to the surface and a vertical block at the anterior (zero mm) end. Place the fish on the board with its head flush with the block and spread the caudal fin to show the mm mark under the anterior point of the fork.

Some fish species such as burbot, sculpins and darters do not have a fork in their caudal fins. For these species, the standard measurement is Total Length, which is the distance from the most anterior part of the head to the distal tip of the longest caudal fin ray.

The fish which must be measured for length and weight may vary between projects. You will always be measuring game species but will not necessarily have to measure rough or forage fish. The project manager will be able to tell you what is required. For instances where large numbers of individuals are being captured and the time required to measure length and weight is excessive, it may be possible to measure length only for some fish. A large number of lengths are required to produce a complete length-frequency distribution (see section 3.25) while a lesser number of weight measurements are required to provide an accurate length-weight analysis (see section 3.26). If fish are being preserved, always measure length and weight before preserving.

3.24 Length-at-Age

Length-at-age analysis is used to determine the average length of fish in each age class in the population. This analysis can only be conducted for individuals for which age is known. For each age class (i.e. 1 year old fish, 2 year old fish, etc.) calculate the range of lengths, mean length and the standard deviation of the mean. Plot this data graphically showing the range, mean and standard error (error bars) (see section 3.47 standard error and standard deviation) with age as the X-axis.

3.25 Length-Frequency Analysis

Length and weight data provide the statistics that are the cornerstone of fisheries research and management. Rate of change of length in individuals and length-frequency distributions are key attributes of fish populations. Length-frequency analyses provide an important description of population structure and are used to provide information for the interpretation of age and growth, especially for young fish. Length-frequency distributions reflect the interaction of rates of reproduction, growth and mortality of the population. However, when interpreting length-frequency data it is important to evaluate sampling biases for the capture technique that was used, particularly with respect to size selectivity. The length-frequency distribution of a population is shown graphically by plotting the number of fish in each size class using a histogram chart. Typically, size classes include every 50 mm fork length interval (i.e. 0-50 mm, 51-100 mm, 101-150 mm..... etc.) but may be more frequent if you have a large sample size. When plotting the length-frequency distribution using Microsoft Excel, label the size classes on the X-axis of the graph using the complete label (i.e. 0-50 mm, not 50 mm).

Using the length-frequency analysis to determine fish age and growth rates is called the Peterson method. The plot of the length-frequency analysis is examined for peaks which are believed to represent each of the vear classes in the population. The peak closest to the Y-axis would represent zero aged fish (young-of-the-year) and each peak after that should represent another year class. Great care must be exercised when conducting age analysis with this technique. Typically, distinct peaks are only evident for the first few year-classes. Individual fish exhibit different growth rates and as they get older, the overlap in size ranges for each age class becomes too great and the peaks in the length-frequency distribution are lost. In addition, this method requires measurement of a large number of fish which represent an unbiased sample of the population. The size intervals (fork length classes) chosen for plotting these data are particularly important, as size intervals which are too large or too small will obscure the peaks. Other problems with this method include dominant year-classes which may obscure the peaks of weaker year-classes and divergent growth rates of male and female fish complicates the analysis as does the small incremental changes in length which occur in older fish. However, the Peterson method is quite suitable for some forage fish populations where the life-span is short. It is the recommended ageing method for some minnow species which may have life-spans as short as three years.

3.26 Length-Weight Relationships

Length-weight relationships can be used in order to assess the state of well-being of a fish population. These relationships can be used to compare the condition or "fatness" of fish in a population to other populations, or to that in previous vears. As a fish population size increases and/or food resources decline, individual fish become thinner and the ratio of weight to length decreases.

The relationship between fish length and body weight is curvilinear, and can normally be represented by the following function:

W = aL^b

where W = weight, L = length, and 'a' and 'b' are constants which are characteristic of the population being examined. The constant 'b' reflects the rotundness of the fish or the rate at which weight increases for a given increase in length. In general, a value of 'b' less than 3.0 represents fish becoming less rotund as length increases, and 'b' greater than 3.0 indicates a population where fish become more rotund as length increases. If 'b' is equal to 3.0, growth is isometric, meaning shape does not change as fish grow.

The length-weight relationship that we typically use is called length-weight regression analysis. The length-weight relationship can be changed from curvilinear to linear (straight line) using a log₁₀ transformation of both length and weight. The relationship between length and weight becomes:

log W = log a + b log L

where log a is the 'Y' intercept of the regression line and b is the slope of the line. A regression analysis can be conducted from length and weight measurements of a sub-sample of the fish population. Be sure to measure fish which are representative of the size range in the population, that is an even number of fish should be measured from all size groups in the population, from the smallest to the largest fish. A general rule is that at least 30 fish should be measured to provide a large enough sample size to calculate an accurate regression. The regression analysis plots the log weight versus log length for all the fish measured and then produces the "best fit" straight line that approximates the mathematical relationship between length and weight. The regression analysis can be conducted by entering the length-weight data on a computer spread sheet (Microsoft Excel) and having the program conduct the log transformation of the data. The computer program will provide the regression equation, including the values for 'a' and 'b'. When conducting a regression analysis, you should also record the 'R' value (coefficient of determination) that the computer calculates as this value represents properties of the linear relationship. The higher the 'R' value, the more closely the data conforms to a straight line and the better the regression equations represents the data.

Differences often exist in the body weight to length relationship for males and females in the same population. If possible, length-weight regressions should be calculated separately for the two sexes. The relationship also changes throughout the annual growing season, particularly for females, as gonad size and weight increases, so care should be taken when comparing various sets of data. Prior to conducting a length-weight regression analysis, the length-weight data should be plotted on a scatter diagram in order to spot 'outlying' data points. Points. Points which are well outside the range represented by the other data points should be checked for accuracy to make sure both length and weight were recorded properly.

3.27 Lesion

Lesions are the result of a pathological change in body tissue. External hemorrhagic lesions (bloody sores) may be observed on the body surface of the fish and should be recorded on the Fish Sample Record form. Reddened areas and lesions on the body surface are evidence of systemic (widespread, internal) infections of bacteria or superficial bacterial infections. Skin lesions in wild fish are seen most often in the early spring when rising water temperatures encourage bacterial growth at a time when fish are least resistant to it. An increased prevalence of skin lesions also has been associated with fish from water with a high organic load and bacterial community, such as below a sewage outfall.

3.28 LSI (Liver:Somatic Index)

Liver-Somatic Index is also known as hepato:somatic index. It is the ratio of liver weight (g) versus total body weight, expressed as a percentage of total body weight. The LSI is used as an indicator of fish health. Energy is stored in the liver in the form of glycogen and the relative size of the liver is believed to correlate with nutritional state.

3.29 Marking/Tagging

Identification of individual fish or simply identification of fish which have been captured is required for some projects. Different marking techniques are available, depending on the goals of the study.

3.29.1 Anchor (Floy) Tagging

A practical and inexpensive method of permanently marking individual fish. The tag, shaped like an inverted "T", is most commonly inserted through the fishes' back at the base of the rear portion of the dorsal fin and anchored between the epipleural bones of the dorsal fin using a special tag-gun. The tip of the gun is a hollow needle which is inserted through the skin and muscle. As the handle of the tag-gun is depressed, an injector rod pushes the anchor portion of the tag out the end of the gun through the needle. The tag-gun needle will not pass through fish scales. In order to insert the needle, use the tip of the needle to lift the posterior edge of a scale and slip it in under the scale. Fully insert the needle through the skin by inserting it to the base of the needle and depress the handle. Once the tag-gun handle has been fully depressed, hold it in the depressed position while giving the gun a quarter turn to free the tag from the needle. Still with the handle depressed, remove the tag-gun needle from the fish and the tag will remain anchored in place.

The posterior portion of the Floy tag remains outside the fishes' body and is usually brightly coloured and carries a numeric identification code. This tagging method is used when conducting mark-recapture population estimates and basic fish movement studies. It is also the preferred marking technique when seeking angler return data to aid in establishing fish movements. Tags marked with the researchers address and the phrase "$2 reward" are often used to ensure angler response.

When sampling, always record the recapture of marked fish, even if the tag is not one that was inserted during your present study. It is common to catch fish carrying old Floy tags inserted by other agencies who will provide the date and location the fish was tagged; information which will provide movement data for all of the researchers involved. Older tags will usually have a build up of algae and will need to be scraped clean with a knife in order to read the tag number and other information.

Floy tags will usually carry the name and address of the client/agency that Golder is working for and, therefore, the tags are usually provided by the client. If this is not the case, Floy tags will need to be ordered and discussion with the client may be necessary to decide what writing the tags will carry.

3.29.2 Visual Implant (VI) Tagging

A "micro-tag" method using tags which are inserted under the skin. VI tags are suitable for use when a tagging method is required which has minimal effects on the swimming and feeding efficiency of the fish. Good for tagging smaller fish than is possible with the anchor tag method, such as small fish species or juvenile fish. Each tag consists of a small metal strip with an individual alpha-numeric code (typically three digits) which is inserted using an injector into a clear tissue somewhere on the fishes body (e.g., post-ocular tissue for salmonids). If working with non-salmonids, it will be necessary to determine a suitable implant location for the fish species you are working with. The implant location should have a sufficiently thick layer of clear tissue so that there will be room to insert the flat injector needle and the tag can be read through the tissue. Record in the field notes the location (including left or right side) of tag insertion for each fish species that you are tagging. To tag a fish, insert the injector needle into the selected tissue, depress the injector and hold it down while removing the needle from the fish.

3.29.3 Batch Marking

A marking method which does not distinguish between individual fish. Common methods are fin clipping or dye marking. Batch marking can be used to distinguish fish from specific sites by varying the location on the fishes' body which is dye marked, the colour of the dye or varying which fin is clipped by sampling site. This method is suitable for simple movement studies and for simple mark-recapture population estimates. This method is also used when extremely large numbers of fish need to be marked, as it is simple and more economical than anchor or VI tagging.

Dye marking is accomplished by injecting a small amount of a coloured dye or liquid plastic sub-cutaneously. It can be used for marking very small fish, such as minnows and other forage fish, since a very small hypodermic needle can be used as the injector. One disadvantage of dye marking forage fish is that it is difficult to avoid using a colour which is readily visible to the researcher without increasing the probability of predation of the marked individuals.

Fin clipping includes removing or distinctively altering a fin in a recognizable manor. Fin removal is usually only conducted for non-essential fins such as the adipose fin on salmonids. For other fins such as the pectoral or pelvic fins, the first two fin rays may be removed. For larger fish, a hole punch can be used to make a distinctive mark on a fin. When clipping a fin, it is important to make straight, regular cuts to distinguish the mark from naturally frayed or eroded fins. Record the fin which is marked for each sampling site.

3.29.4 Radio Tagging

Attachment of a battery powered radio transmitter to a fish in order to follow its movements using a radio telemetry receiver. The transmitter is affixed externally or surgically implanted in the body cavity. To avoid adverse effects on swimming ability, the transmitter should be <2% of the fishes' body weight. Ground. boat or aerial surveys are conducted with the telemetry receiver in order to follow the fishes movements.

3.30 Maturity (State-of-Maturity)

Maturity refers to the state of gonad maturation of an individual fish at the time it is examined. It does not refer to whether or not the fish is "mature" (i.e. adult); classification of a fish as juvenile or adult is referred to as life-history stage (see Section 3.46).

For adult fish, the gonads will typically progress through a series of conditions or phases of maturation each year during the seasonal development cycle. Although juvenile fish have only one possible state-of-maturity, adult fish can be one of several maturities. The state-of-maturity is used to determine the current reproductive status of the individual. For fish populations, state-of-maturity data can be used to determine the size or age at first spawning, the proportion of the stock that is reproductively active, or to illustrate the nature of the reproductive cycle.

Golder uses a system that includes 9 maturity categories. The 9 categories, their definitions and abbreviation codes are presented on the back of the Fish Sample Record forms used to record the data. More detailed definitions and descriptions of each maturity category, for both males and females, are provided in Appendix I. Maturity is best determined by conducting an internal examination of the gonads, which requires sacrificing the fish. Maturity can sometimes be determined by external examination of the fish based on fish size and by knowing the typical spawning period for the fish in relation to the capture date or, for some species, by external secondary sexual characteristics which become pronounced during the spawning season (see Section 3.41). The classification system includes an "unknown" category for fish which are examined externally and for which maturity cannot be determined.

For many studies, most or all fish will be released live and only external examinations will be conducted. For other studies, a sub-sample of fish captured will be sacrificed for definitive state-of-maturity data. The following are some hints for establishing state-of maturity from external examination. Pre-spawning fish will be found immediately prior to the species spawning season. Fish of a size large enough to be adult or displaying secondary sexual characteristics at this time and with a strongly distended body cavity may be Pre-spawning. During the spawning season, gametes (milt or roe) can be extruded from the fish with gentle pressure on the abdomen and it will be obvious that the fish is Ripe. Spent female fish can be identified by a flaccid, concave abdomen resulting from shedding of the large egg mass and abdominal abrasions obtained during spawning activity. They may extrude a small number of residual eggs in response to pressure on the abdomen. Spent males may also have abdominal abrasions and will probably still extrude milt with abdominal pressure, but the milt may appear "watery". Other maturity classifications are very difficult to determine from external examination.

3.31 Milt

Milt is a milky white fluid extruded by male fish during spawning activity and contains the sperm. During spawning season, ripe male fish will extrude milt in response to pressure on the abdomen.

3.32 Necrosis

The death of a tissue due to injury or disease.

3.33 Parasites

Fish are subject to several types of internal and external parasites. A complete parasitological examination requires sacrificing of the subject and microscopic examination of some tissues. For general fisheries inventories, the occurrence of macro-parasites which can be readily observed by the an-aided eye should be recorded on the Fish Sample Record Form. A basic external examination is conducted while measurements of length and weight are conducted. An internal examination is conducted for fish which have been sacrificed. Common external parasites include body lice, gill lice, leeches and lamprey. Common internal parasites include tapeworms, nematodes and flukes associated with the gastro-intestinal tract and other internal organs.

3.34 Pathology

For fisheries inventory studies, pathology refers to the field examination of captured fish for indications of parasites, disease and abnormalities, without the use of special procedures (e.g. tissue collection) or tools (e.g. microscope). This can include either external pathology or external and internal pathology.

External Pathology

Examination of the body surface, fins, eyes, gills and gill chamber for signs of parasites, disease or abnormalities (deformations). Components of the external examination include body form, body surface, lips and jaws, snout, barbels, opercles, isthmus, eyes, fins, gills, pseudobranch, branchial cavity, anus, and the urogenital opening. A basic external examination can be conducted for most fish while measurements of length and weight are being conducted and the results recorded on the Fish Sample Record Form.

Internal Pathology

Examination of the body cavity and internal organs for signs of parasites, disease and abnormalities. Components of the internal examination include body cavity, mesenteric fat, liver, gall bladder, hind gut, stomach, pyloric caeca, intestines, spleen, gas bladder, kidney, gonads, and muscle. A bsic internal examination can be conducted for fish which have been sacrificed.

3.35 Population Estimates

Population estimates are used to determine or approximate the total number of fish, for one species or a number of species, within a study area. Population estimates may be calculated for a portion of a waterbody (e.g. a section of stream - #fish/km) or an entire waterbody (e.g. a lake - #fish/ha). Two basic types of population estimates are used; Removal and Mark-Recapture.

Removal (Reference - Armour et al. 1983)

Removal population estimates involve the isolation of the study area using a physical barrier to block fish movements followed by the removal of fish from the area to provide a population estimate. This technique is restricted to study areas which can be isolated and is typically used in small streams. Small-mesh blocking nets are placed at the upstream and downstream boundaries of the study area to prevent immigration or emigration of fish from the study area. Long minnow seine nets area used as blocking nets and are held in place using rebar posts embedded in the substrate. Care must be taken to ensure the bottom of the net remains in contact with the stream substrate to form an effective barrier.

Electrofishing is used used as the capture technique, typically backpack or portable boat electrofishing, depending on stream size and water depth. It is vital that the capture technique be very efficient. If the stream is too deep or wide for effective sampling by backpack electrofishing, the portable boat electrofisher should be used or use two backpack units working simultaneously. Multiple electrofishing passes are conducted within the study area and the catch (species and length) and sampling effort are recorded for each pass. Captured fish are retained in a holding pen or are released outside the study area. The catch will decline with each pass as the number of fish in the study area is reduced. Ideally, the catch on the final pass will be zero as total removal is achieved, however, total removal is not required. What is required is that the capture efficiency must be high enough that the probability of capture for each individual is high. When this requirement is met, most of the fish in the study area will be captured on the first pass. After two electrofishing passes, the capture probability is calculated (Armour et al. 1983). If the capture probability is 0.8 or greater, the capture efficiency is high enough to provide an accurate population estimate and a sufficient number of passes has been conducted. In practice, capture probabilities as high as 0.8 are uncommon and additional passes must be conducted. Typically, 3 or 4 passes must be conducted to get a good estimate of capture efficiency and to get enough data to calculate a population estimate. If after 4 passes the number of fish beign captured has not declined to near zero, the sampling technique is not sufficiently effective and the population estimate will have poor accuracy. A population estimate can be calculated from such data, but the confidence intervals will be very large.

It is very important that the diminishing catch on subsequent passes be due to the reduced number of fish in the study area and not to a reduced amount of sampling effort. It is vital that a similar effort be expended on all passes. The number of seconds of electrofishing and the search pattern in the study area should be similar for all passes. Monitor the electrofishing seconds throughout each pass in order to ensure this requirement is met.

If total removal is achieved, the population estimate for each species is equal to the total number of individuals captured. If total removal is not achieved, formulas are used to calculate the population estimate. Two formulas are available; the first is a simple formula for computations for two removal passes and the second is more complex for computations for more than two removal passes (Armour et al. 1983). Both of these formulas are presented on a Microsoft Excel spreadsheet in the G:\Aquatics directory. Simply type in your data for each species (i.e. number of fish captured each pass) and the spreadsheet will calculate capture probability, population estimate, standard error and the 95% confidence interval. The lower limit for the 95% confidence interval is sometime lower than the number of fish that was captured. If this is the case, the lower limit should be changed to equal the number of fish captured as this mumber represents the minimum population size.

Mark-Recapture

Mark-recapture population estimates are used in situations where isolation of the study area is not possible or for situations where removal of a significant portion of the population is not practical. Using this technique, a sub-population of fish is captured, marked and released. These fish are then allowed to mix with the larger unmarked population. A sub-sample of fish is then captured and the number of marked and unmarked fish is used to determine the proportion of the total population represented by the marked sub-population. As the size of the marked sub-population is known, the size of the total population can be calculated. This technique is useful in large and intermediate sized streams and in lakes. Any sampling technique with good sampling efficiency can be used but is typically limited to electrofishing, particularly in flowing waters. The mark-recapture technique assumes a closed population (no immigration/emigration) which is not usually true in many situations. Study design should include aspects to reduce the effects of immigration/emigration of fish. For size selective sampling techniques such as electrofishing, population estimates should be conducted separately for different size classes.

For most mark-recapture population estimates, it is recommended that multiple sampling passes be conducted to capture and mark fish. This is followed by a few days without sampling to allow mixing of marked fish in the general population. A sampling pass (census) is then conducted to determine the portion of marked to unmarked fish in the census sample. Batch marking (see section 3.29) can be used for this technique. The population estimate is calculated using the Chapman modification of the Peterson method (Ricker 1975) as follows:

N=(M+1) (C+1) / R+1

where N = population estimate, M = number of marked fish, C = sample taken for census, and R = number of marked fish in the census sample.

At Golder we generally use the CAPTURE program (Otis et al. 1978) for mark-recapture population estimates. For this method, the fish marking technique must be Floy or VI tagging (see section 3.29) as each individual fish must be indentifiable. Multiple sampling events are conducted in order to tag fish and to keep daily counts of the number of tagged and untagged fish that are captured. The results are then arranged in a matrix which has one line for each individual fish that was captured, along with the day or days it was captured tagged and recaptured. This matrix is used by the CAPTURE software to provide the population estimate. The CAPTURE program is located in the G:\Aquatics directory. The CAPTURE software tracks the capture/recapture history for each individual fish over each pass and calculates the population estimate based on these results. This technique is believed to provide a more accurate result than the single census-pass estimate presented above. This technique does not require a rest period between the marking passes and a census pass and is more suitable for use in open populations where fish movements in or out of the study area may occur.

3.36 Riparian

With respect to fisheries habitat evaluations, riparian areas are terrestrial habitats bordering water bodies (lakes and streams). Riparian area are not included within the boundaries of the waterbody but are significant in providing habitat features such as overhanging vegetation, inputs of large-woody-debris, sediment stabilization, shading, moderation of surface water run-off, nutrient inputs, etc. Riparian conditions, including species of bank vegetation and floodplain vegetation when possible, are an important part of habitat evaluations.

3.37 Roe

Fully developed, unfertilized eggs produced in the ovaries of adult female fish. During spawning season, ripe female fish will extrude roe in response to presure on the abdomen.

3.38 Rough Fish

Large fish species (i.e. non-forage fish) which are not included as game fish. Primarily sucker species.

3.39 Sacrifice

Fish which are killed in order to allow internal examination or collection of ageing structures are referred to as sacrificed. For each fish captured, information on whether or not the fish was sacrificed is recorded on the Fish Sample Record Form (i.e. capture code), which helps to identify fish which have been examined internally versus those which were only examined externally. Fish which are sampling mortalities (accidentally killed as a result of capture) are also recorded as sacrificed. Even if intentionally sacrificing fish is not a part of the study design, dead fish should be examined internally for definitive sex and state-of-maturity data, as well as stomach contents and internal pathology when time allows.

3.40 Sampling Bias

Sample inaccuracy caused by bias or imprecision in sampling; e.g., bias towards large fish because of the type of sampling gear. In statistics, a sampling bias may be represented as skewedness or as variance.

3.41 Sex

Sex refers to the sex of the individual fish, usually recorded as either male or female. However, since determination of sex may be difficult from external examination or from internal examination of juvenile fish, sex may aslo be recorded as unknown.

Sex Determination (Lethal)

To determine the sex of a fish, an incision should be made on the ventral surface of the body from a point immediately anterior of the anus toward the head to a point immediately posterior to the pelvic fins exposing the gonads. If necessary, a second incision may be made on the left side of the fish from the initial point of the first incision toward the dorsal fin. To observe the gonads, fold back the tissue. Ovaries appear whitish to greenish to orange and have a granular texture. The eggs will be readily apparent in developed ovaries. Testes appear creamy white and have a smooth texture.

Sex Determination (Non-Lethal)

Determination of sex from external examination of the fish is generally more difficult. For some species, sex may be determined from external secondary sexual characteristics, observable either during the spawning season or, for some species, at any time of year. For most fish species, sex of adult fish can be determined during the spawning season by forcing extrusion of the sexual product (milt/roe).

Secondary sexual characteristics are external physical characteristics displayed by fish which distinguish sex. Some species do not display secondary sexual characteristics. Other species show secondary sexual characteristics during the spawning season and these characteristics are only useful for distinguishing sex for adult fish during the spawning season. Still other species have morphological differences which allow determination of sex from external examination at any time.

Mountain whitefish develop small tubercles (raised bumps) on the lateral scales prior to spawning. These tubercles are generally more pronounced in males than in females but, alone, tubercles may not be a reliable indicator of sex. Trout may show differences in jaw morphology with females having a rounded jaw and male developing a kype (extended, upwardly hooked lower jaw). This characteristic is not reliable in that the male may not develop a kype, particularly in smaller adults. Males for most sucker species develop obvious tubercles which show as hard nodules in the pelvic, lower caudal and, particularly, the anal fin during the spawning season and which are very reliable for determining sex in adult fish. Many species, such as minnows, suckers and some trout develop distinct body coloration or markings during the spawning season which may aid in separating the sexes. Two species, goldeye and mooneye, show a difference in anal fin structure between mature male and female fish which is a reliable external indication to distinguish sex at any time. In the female, the longest rays of the anal fin are the first four and all of the anal fin rays are slender. The overall shape of the fin is "smoothly concave". The first half of the anal fin of the male has long rays followed by much shorter rays at the back, giving the fin a "lobed" appearance. In the male, the anterior rays are thick near the base. This characteristic is not reliable for juvenile fish.

3.42 Spawning Surveys

Spawning surveys refer to the visual observation of spawning activity or sampling for the presence of incubating eggs and are used to determine if a site has been used as a spawning area, to determine the distribution of spawning sites within a study area, or to collect micro-habitat data (Habitat Preference Criteria) at known spawning areas. Spawning occurs when eggs (roe) and milt (sperm) are extruded by the fish so as to mix and produce fertilized ovum. This is accomplished in a number of ways by different species. Most game fish species for which spawning surveys are typically conducted are either spring or fall spawning species. There are two basic types of spawning surveys (egg surveys or redd surverys) depending on the spawning strategy of the species involved.

Egg Surveys

Some species, such as mountain whitefish, lake whitefish, lake trout, walleye and sauger are broadcast spawners which distribute their eggs over the substrate in areas of suitable depth, velocity and substrate type. The eggs fall into the interstitial spaces (crevices) in the substrate to incubate, although some species will spawn over hard sand if rocky substrates are not available. Spawning surveys for broadcast spawners are conducted using kick sampling and/or airlift sampling techniques (see sections 3.5.1 and 3.5.9). If the study area is small, systematic sampling can be used to examine the entire area for eggs. In large study areas where this type of sampling is impractical, sampling is conducted by examining areas of suitable spawning habitat for the target species. Habitat preference information (see section 3.22) is used to determine the habitat types that should be examined. The section of the stream or portion of lake that is examined during the survey and the location of all spawning sites where incubating eggs are recovered should be identified on maps of the study area. The standard is to use 1:50,000 scale topographical maps but other maps or air photos may be used if they provide greater accuracy. The number of eggs recovered is also recorded for each spawning site and, depending on the sampling technique, sampling effort may also be recorded at each site.

If incubating eggs are found in a study area where more than one species may be spawning, measure egg diameter for the recovered eggs and use egg size, colour and features such as the presence or absence of oil globules to identify the eggs. Egg diameter can be measured using an egg measuring trough. Place 10 eggs in the trough and measure the total amount of the ruler covered, divide this distance by 10 to get an average egg diameter. Scott and Crossman (1973) provide egg descriptions for most species. If egg identification is still doubtful, Collect a sample of eggs, measure the gee diameter, and preserve the sample in 5% buffered formalin.

Some fish species use spawning strategies which are part-way between broadcast spawners and species which construct spawning nests. These species include Arctic grayling and several sucker species such as longnose and white sucker. No actual nest or redd is prepared but spawning occurs close over the substrate while the fish are vigorously vibrating and the fertilized eggs become somewhat covered by the substrate material stirred up during this vibration. In some cases, such as spawning areas used by a large number of suckers, disturbances of the substrate can be visually observed but it is not possible to enumerate the number of spawning acts or the number of fish involved. For species such as Arctic grayling, these disturbances are indistinct. Spawning surveys for these species are conducted using egg surveys, as for broadcast spawners.

Still other species, such as northern pike and yellow perch, attach their incubating eggs to submerged vegetation (aquatic macrophytes or flooded terrestrial vegetation). Spawning surveys for these species are conducted by searching for eggs in areas of submerged vegetation. A kick sampling net or other small mesh net is swept through the vegetation and the net contents are examined for eggs.

Redd Surveys

Most trout species (including brook, brown, bull, cutthroat and rainbow trout) construct excavations in the substrate into which the fertilized eggs are deposited. A similar excavation immediately upstream of the depression is dug and the materials from this excavation are used to cover the incubation eggs. These excavations or spawning "nests" are termed redds and are typically constructed in flowing water, although areas of ground-water upwellings in lakes may also be used. As the algae and silt covered rocks are turned over during redd construction, the redds can usually be readily observed due to their "clean" nature and distinctive shape (i.e. distinct depression upstream of a mound). Redd surveys are conducted by one or more observers walking or floating through a study area, enumerating the redds observed, and recording the locations of the redds on a 1:50,00 map of the study area. The study area (section of stream or portion of lake) examined should also be recorded on the map. Not all excavations are redds which contain incubating eggs and it may sometimes be difficult to determine if a disturbance of the streambed is truly a redd. Therefore, redds should be enumerated and classified into the following categories: 1) Class A redd - large or distinct, well formed or spawning fish present; 2) Class B redd - less distinct, most likely an active redd; 3) Class C redd - small or indistinct, possible redd but not definite.

If more than one trout species may be spawning in the study area, enumeration of the redds by species may be difficult. If this is the case, species identification for each redd is best facilitated by conducting the redd survey during the active spawning period so that it is likely that the fish will be present at the redds to aid in identification. Knowing the species and size of the fish in the study area will also help, as some species build larger redds than others. If only one species is expected to be spawning in the study area, the redd survey is usually conducted towards the end of the spawning season when the maximum number of redds will be present.

Repeated redd surveys in the same study area can be used to define the spawning season if required. Surveys are conducted at regular intervals from the start of the spawning season and the number and location of redds on each successive survey is used to determine the length and peak of spawning activity.

3.43 Species Code

Standard abbreviation of fish species names is based on the following rules (MacKay et al. 1990):

use a four letter abbreviation
for a one word name - use the first four letters

e.g., GOLD for goldeye
two word names - use the first letter in each word plus the next consonant in each word

e.g., ARGR for Arctic grayling,

LKWH for lake whitefish, and,

WHSC for white sucker

(exception - due to duplication, use BRTR for brook trout and BNTR for brown trout)
three word names - use the first letter in the first two words and the first letter and next consonant in the last word

e.g., NRDC for northern redbelly dace

The species codes for all Alberta species are presented on the back of the Fish Sample Record Form.

3.44 Species Composition

A term that refers to the species found in the sampling area.

3.45 Species Distribution

Where the various species in an ecosystem are found at any given time. Species distribution varies with season and life history stage.

3.46 Stage (Life History Stage)

Stage refers to the life history stage (or life stage) of the individual fish. Three stage categories are used to describe free swimming fish: fry, juvenile or adult. The incubating egg is also a life stage and is referred to as the embryo stage.

Fry are also called young-of-the-year (YOY) and are fish from their hatching date until the first anniversary of their hatching date. Juvenile fish are fish from one year old until reaching sexual maturity. Adult fish are fish which are sexually mature.

Definitive life history stage is determined for an individual by internal examination of the gonads. Fry and juvenile fish would have undeveloped gonads and would be classified as immature with respect to state-on-maturity. Fry can usually be separated from juvenile fish by their small size (i.e. smallest fish in the population) and, for some species, by secondary characteristics such as parr marks. Adult fish are sexually mature fish which have spawned in the past or will spawn in the upcoming spawning season. Their state-of-maturity can be one of several categories, from maturing to spent.

Determination of stage from external examination is not always possible. Identification of fry is based on their small size. However, it is not always possible to tell large juvenile fish from small adult fish, in which case an unknown category is provided in addition to the three main categories. Evidence of sexual maturity, such as secondary sexual characteristics or extrusion of milt or roe during the spawning season can be used to identify adult fish.

3.47 Standard Error and Standard Deviation

Standard error (SE) and standard deviation (SD) both express the variability of results around the mean. However, standard error takes the sample size into consideration when calculated. By including sample size, SE gives an indication of how well we've measured the entire population. This is particularly true if you have very different sample sizes for the groups you are comparing; the larger the sample size, the more confidence you have that the data represents the population.

Standard error is calculated as: SE=SD ÷ ?n; where n=sample size. Microsoft Excel will calculate SD automatically. In order to calculate SE the formula in Excel would be "=StDev(cells with data)/(sample size)^ 0.5". The "^.05" denotes square root (by asking excel to calculate to the power of 0.5).

Standard error is now considered to be the appropriate measure to use in any technical presentation of data and should be used in any figures or tables of fish population statistics.

3.48 Stomach Content/Gut Analysis

Stomach content analysis is used to determine the diet and food preferences of fish. The stomach is removed from the sacrificed individual and opened to allow examination of its contents. Record stomach fullness as the percentage of fullness, from 0 to 100% Record the contents of the stomach as percentage of the material in the stomach, not as percentage of the total stomach volume (e.g. a stomach that was half full, with all the contents being mayflies would be recorded as follows: 50% full, 100% mayfly).

For invertebrates in the stomach contents, record the contents to the lowest taxonomic level possible. Family level is usually required, but Genus should be recorded if known. Unidentifiable, overdigested invertebrates should be recorded as IR (invertebrate remains) and unidentifiable fish remains should be recorded as FR (fish remains).

3.49 Study Site/Sampling Location

A study site or sampling location is the portion of a study area at which sampling is conducted. The site may be a point location (such as a gill net or set line location) a transect (cross section of a stream channel or lake) or a section (such as a section of stream electrofished or an area of a lake which is seined). In any event, the location of the sampling site must be recorded in the field notes. For large studies or studies with multiple sampling locations on the same waterbody, you may wish to number each sampling site. For a single waterbody, sample site may be numbered sequentially (i.e. #1, #2, etc.). For multiple waterbodies, you may wish to combine the number with an abbreviation for the waterbody (e.g. BRI = Bow River Site #1). You may also wish to identify the type of sampling conducted (e.g. GNI = gill net set #1). All study site abbreviations must be clearly identified in the field notes. At a minimum, all study sites should be recorded on a 1:50,000 scale topographical map. Other maps or air photos may also be used if they provide greater detail than the 1:50,000 map. See section 3.17 for additional methods of recording location.

Study areas on flowing watercourses are often divided into homogeneous sections called reaches. a reach is a relatively homogenous section of stream having a uniform set of characteristics and habitat types. A reach is relatively uniform with respect to channel morphology, flow volume, gradient and habitat types and is separated from other reaches by changes in these characteristics. Conventionally, reach numbers are assigned in an upstream ascending order starting from the mouth of the stream. Typically, reach lengths are too long to sample in their entirety, in which case representative study sections will be selected in each reach for determining species distribution and abundances.

3.50 Temperature Criteria

Water temperature is a very important habitat component. Different fish species have different temperature requirements and have different tolerances to high water temperatures. Temperature regime in lakes and rivers can affect the presence, distribution and abundance of fish species (see Sections 3.7 and 3.9). Temperature criteria provide maximum temperature levels that are tolerable by various life stages and have been developed for selected game fish species. Golder has prepared a document which list the criteria for selected Alberta species (Taylor and Barton 1992).

3.51 Underwater Video

Underwater video equipment includes a remote control underwater camera, light and above surface monitor and video recorder. Underwater video is used to determine fish presence, general abundance and activity. It is not generally useful for recording fish numbers. It is a sampling technique that is effective in both the open water season and for winter sampling under the ice.

3.52 Water Quality

Water quality is a basic aspect of fisheries habitat and can influence fish survival, distribution, abundance and reproductive success. Basic water quality parameters that are measured for fisheries studies include; temperature, dissolved oxygen, PH, conductivity, visibility (secchi depth), turbidity, total suspended solids (TSS) and total dissolved solids (TDS).

3.53 Weight

Weight refers to the total body weight (wet weight) of fish. It is measured for live fish before they are released or for sacrificed fish immediately after they have been killed. Along with length, weight is one of the most basic parameters measured evaluate the key attributes of fish populations.

Weight should be measured in grams (g) using a properly calibrated dial scale or electronic scale, depending on fish size. Golder uses dial scales fitted with fork length troughs for measurements of intermediate and large fish. Two types of dial scale are used; small scales which are rated for 0-4 kg in weight are used for most fish species, large scales rated for 0-25 kg are used for large fish species. For forage fish species and fry life stages of large fish species, more sensitive digital electronic scales are used.

3.54 Weight-at-Age

Weight-at-age analysis is used to determine the average weight of fish in each age class in the population. This analysis can only be conducted for individuals for which age is known. For each class (i.e. 1 year old fish, 2 year old fish, etc.) calculate the range of weights, mean weight and the standard deviation of the mean. Plot this data graphically with age as the X-axis, showing the range, mean and standard deviation (error bars). Weight -at-age is usually plotted on the same graph as length-at-age data.

4 REFERENCES AND SUGGESTED READING

Anderson, R.O. and S.J. Gutreuter. 1983. Length, Weight and Associated Structural Indices. In: Fisheries Techniques. L.A. Nielsen and D. Johnson (eds.). American Fisheries Society, Bethesda, MD. Pp. 283-300.

Armour, C.L., K.P. Burnham, and W.S Platts. 1983. Field methods and statistical analysis for monitoring small salmonid streams. U.S. Dept. Interior., Fish Wildl. Serv. FWS/OBS-83/33. 200 pp.

Carlander, K.D. 1969. Handbook of Freshwater Fishes of the United States and Canada. 3rd Ed. Iowa State University Press, Ames, I.A.

Hayes, M.L. 1983. Active Capture Techniques. In: Fisheries Techniques. L.A. Nielsen and D.L. Johnson (eds.).

American Fisheries Society, Bethesda, M.D. pp. 123-146.

Jearld, A. 1983. Age determination. In: Fisheries Techniques. L.A. Nielsen and D. Johnson (eds.). American Fisheries Society, Bethesda, MD. Pp. 301-324.

MacKay, W.C., Ash, G.R., and H.J. Norris (eds.). 1990. Fish Ageing Methods For Alberta. R.L.&.L. Environmental Services Ltd. in assoc. with Alberta Fish and Wildlife Div. and Univ. of Alberta, Edmonton. 113 p.

Nelson, J.S., and M.J. Paetz. The fishes of Alberta (2 ed.). The Univ. of Alberta Press.

Nielson, L.A., and D.L. Johnson. 1983. Fisheries techniques. American Fisheries Society, Bethesda, Maryland.

Otis, D.L., K.P. Burnham, G.C. White, and D.R. Anderson. 1978. Statistical inference from capture data on closed populations. Wildl. Monogr. 62. 135 pp.

Ricker, W.E. 1975. Computation and interpretation of biological statistics of fish populations. Dept. of Env., Fish. and Marine Serv., Bulletin 191, Ottawa.

Schreck, C.B., and P.B. Moyle. 1990. Methods for fish biology. American Fisheries Society. Bethesda, Maryland.

Scott, W.B. and E.J. Crossman. 1973. Freshwater Fishes of Canada. Bulletin #184, Fisheries Research Board of Canada, Fisheries and Oceans, Ottawa, Ontario. 966 p.

Taylor, B.R., and B.A. Barton. 1992. Temperature and dissolved oxygen criteria for Alberta fishes in flowing water. Prepared for Alberta Fish and Wildlife Division, Edmonton, Alberta. 72 pp.

5 DISCUSSION

All basic aspects of each fisheries sampling program should be clear before commencement of field work. The field supervisor and field crew should be appraised by the project manager of all study design details. This will include study objectives, delineation of the study area, sampling techniques, data requirements and budgeting. Conditions at the field site may require alteration of the study design. The field crew should act in coordination with the project manager regarding changes to sampling protocols.

APPENDIX I

MATURITY CODES AND DEFINITIONS

UNKNOWN (UN): This category is used when state-of maturity cannot be determined. This will most often occur for fish which have only been examined externally, where no examination of the gonads has been conducted. It may also be used following internal examination of the gonads when the observer cannot definitely determine the maturity of the fish. The gonads have been examined but the observer is unsure which maturity category to use, or the conditions of the gonads do not appear to match any of the maturity categories. If this is the case, record a complete description of the gonads and, if possible, collect a sample for microscopic examination.

IMMATURE (IM): This category is for immature fish (fry or juvenile life stages); defined as fish which have never spawned before and will not spawn in the coming spawning season. The gonads will be undeveloped and will be small and largely transparent. They will be string-like organs situated on the dorsal surface of the body cavity (dorsal to other internal organs) and will lie close under the vertebral column. In very young or small fish, determination of sex from examination of the immature gonads may be difficult or impossible.

Male: The testes will typically be smooth in texture and yellow, pink or white in colour. In suckers and percids, immature male testes can be identified by the position of the testicular artery. The artery is usually totally or partially imbedded in the organ.

Female: The ovaries will typically have a granular texture and will be yellow or pink in colour. In suckers and percids, immature female ovaries can be indentified by the position of the ovarian artery. The artery is usually completely outside the organ, resting on top of the surface tissue and attached with connective tissue.

MATURING (MA): A maturing fish is a fish which has not spawned before but will spawn in the coming spawning season. This category refers to a fish whose gonads are developing for the first time. Fish in the maturing category are, for the first time, considered adult fish as they are hormonally similar to sexually mature individuals. Since the gonads are developing for the first time, development may not be complete at time the fish is examined. The gonads may be developed (enlarged and showing sperm or egg development) primarily at the anterior end. The posterior end of the gonad may still be undeveloped and appear thinner (similar to an immature gonad). This category can be difficult to interpret in the field, being difficult to tell from the Green category, and examination of the gonads by microscope may be required. In general, the gonads of the maturing fish will be smaller than those for aGreen fish.

Male: In the field, maturing testes will be smaller and paler than those of fully developed males but considerably larger than immature testes. If unsure, take a sample for histological analysis and designate the fish as Green (GN).

Female: In the field, maturing ovaries will be smaller and paler than those of fully developed females but considerably larger than immature ovaries. If unsure, take a sample for histological analysis and designate the fish as Green (GN).

SEASONAL DEVELOPMENT (SD): Fish in this category are sexually mature adults which have spawned in one or more previous spawning seasons and will spawn in the coming spawning season. The gonads are undergoing their seasonal development following the last spawning season. This is the longest of the sexually mature stages as it extends from just after the post-spawning period until the next pre-spawning period, as the fish utilizes its resources to produce new gametes. For spring spawning fish (e.g. walleye, northern pike, longnose sucker, rainbow trout, etc.), this category would last from late May to early April of the next year. For fall spawning fish (e.g. lake whitefish, mountain whitefish, bull trout, brook trout, etc.) this category would last from the end of the fall spawning season one year (September to November) through to the fall of the next year. However, for most fish, gonadal development during the winter months.

Male: The testes will vary greatly in size and colour within this category depending on the time of year the fish is examined. Early in development (i.e. after the post-spawning period), the testes will be small and yellow to light orange in colour. By early fall (i.e. after the primary gonad development period in the summer), they will have grown to nearly mature size and be white in colour. At this point, the testes will be large and distinct. Note: Suckers have a black coloured testicular membrane which may mask the white colour of the testes.

Female: The ovaries will vary greatly in size and colour within this category depending on the time of year they are sampled. Early in development (i.e. after the post-spawning period), the ovaries will be small and yellow to light orange in colour. Developing oocytes will be small and dark orange in colour and will give the ovary a granular appearance. By early fall (i.e. after the primary gonad development period in the summer), the ovaries will have grown considerably to nearly mature size and be bright yellow to orange in colour. The individual eggs will be readily apparent.

PRE-SPAWNING (PR): Fish in this category are sexually mature adults which have spawned in one or more previous spawning seasons and will spawn in the coming spawning season. The Pre-spawning category follows right after the Seasonal Development, with respect to both time and stage of gonadal development, and occurs when the gonads have completed their seasonal development prior to the spawning season. This is a short term condition which extends from time the gonads are fully developed until the start of spawning activity.

Male: Externally the abdomen will be slightly distended. Semen can sometimes be extruded with pressure to the abdomen. If this is the case, small amounts of loose semen will be extruded followed by more viscous semen if pressure is re-applied. Internally, the testes will be large and white and will fill much of the body cavity. Pre-spawning condition can also be inferred by the capture location of the male. Males will usually only enter spawning condition once they are on the spawning season approaches is most likely still in pre-spawning condition, even if some sexual products can be extruded. Note: Semen can be extruded from sexually mature males as early as February in spring spawning species.

Female: Externally the abdomen will be noticeably distended. Sometimes a few eggs can be extruded with strong pressure to the abdomen. Care must be taken when applying pressure as the eggs are difficult to extrude and injury to the female can occur. The abdomen will feel tight and hard. Internally, the ovaries will be large and bright yellow to bright orange in colour. The size can be up to 25% of the total body weight and the gonads will fill much of the body cavity. Individual eggs will be large. round and obvious, some eggs will be translucent. Pre-spawning condition can also be inferred by capture location. Females will usually only enter spawning condition once they are on the spawning grounds and around mature males. Thus a female caught away from the spawning grounds as the spawning season approaches is most likely still in pre-spawning condition, even if some sexual products can be extruded.

RIPE (RP): Fish in this category are sexually mature adults. Ripe is the term for the spawning condition. The Ripe category follows right after the Pre-spawning category, with respect to both time and stage of gonadal development, and occurs when the gametes (semen and eggs) have become loose in the gonads. This is a short term condition which extends from start to the end of spawning activity. Externally the fish will appear as they do during the Pre-spawning stage but extrusion of the gametes will occur in response to slight pressure on the abdomen.

Male: Externally the abdomen will be slightly distended. Semen can be extruded with light pressure to the abdomen. Large amounts of loose semen will be produced if pressure is applied. Internally, the testes will be large and white.

Female: Externally the abdomen will be greatly distended. Eggs immersed in ovarian fluid can be extruded with light pressure to the abdomen. Large amounts of loose eggs will be produced if pressure is applied. Internally, the ovaries will be large and yellow or orange. The eggs will be large and translucent and some will appear to be loose as the ovarian tissue is weak (i.e. the ovarian sac will be transparent and thin). Eggs will be loose inside the sac and they will be immersed in clear ovarian fluid.

SPENT (SP): Fish in this category are sexually mature adults. Spent is the term for the post-spawning condition. The Spent category follows right after the Ripe category, with respect to both time and stage of gonadal development, and occurs following spawning activity when the gametes (semen and eggs) have been largely extruded during spawning. This length of time a fish will spend in this category depends on how long it takes for the fish to begin the next cycle of seasonal gonadal development, at which time the fish will again be classified as Green.

Male: Externally, the abdomen will be slightly flaccid, especially ventrally. Some semen can still be extruded with pressure to the abdomen but it will most likely be watery (i.e. not as intense a white colour as in spawning males). Internally, the testes will be reduced in size and gray to creamy-white in colour. Hemorrhaging and distended blood vessels on the surface of the organ are common. Post-spawning males are known to say on the spawning grounds for some time (up to 2 weeks) so capture location is not always a reliable indication of whether the fish has finished spawning.

Female: Externally, the abdomen will be noticeably flaccid, especially ventrally. The surface of the abdomen may be red or roughed with abrasions and the urogenital opening may be extended or swollen. Some eggs can still be extruded with pressure but will be few in number and they will be associated with watery ovarian fluid. Internally, the ovaries will be greatly reduced in size and dark orange to brown in colour. Hemorrhaging and distended blood vessels on the surface of the organ as well as within it are very common and normal. Some residual eggs (from a few up to 25% of the ovary volume) are common. It is not common for post-spawning females to stay on the spawning grounds, most spawn and leave the area immediately. However, capture location is not always reliable indicator.

REABSORBING (RB): Fish in this category are sexually mature fish which have developed to some extent for the coming spawning season but, instead of completing gonadal development or instead of spawning after completing gonadal development, these fish are reabsorbing materials from the gonads back into the body. This category represents arrested gonadal development or interrupted spawning activity. There are several reasons why a fish may terminate gonadal development or decide not to spawn after completing gonadal development. These include the condition of the fish with respect to nutrition and/or health, aspects of population dynamics or environmental cues such s improper water temperatures, poor water quality conditions or adverse water level conditions. Interrupted gonadal development can occur at any stage of development and prior to entering the reabsorbing category the fish may have been Maturing, undergoing Seasonal Development or in Pre-spawning condition.

Male: This condition is extremely rare in males and difficultto observe as reabsorption of the semen by the testes is usually a rapid process. Very rarely will a case be observed of a male actually retaining the entire contents of the testes for re-absorption. Should you suspect this condition the testes should be preserved and stage verified by a qualified biologist.

Female: This condition is primarily observed in females. Reabsorption of the eggs by the ovary is usually a lengthy process which can take up to a full year. Some females may retaining the entire contents of the ovaries for re-absorption. Identification of this stage is not always easy. Externally, the female will still have a distended abdomen if caught within a few months of the spawning season. The abdomen will feel unusually hard as compared to normally developing females. Later in the season, it will be impossible to distinguish a normally developing female from a reabsorbing one without an internal examination. Internally, reabsorbing ovaries go through a series of distinct stages. Early in the reabsorption process, the ovary is dark orange to brown in colour. The eggs are dark and flaccid. Heavy amounts of watery ovarian fluid collect at the posterior of the ovary. This fluid most often is ejected readily if the fish is handled. Later, the ovary becomes smaller and hard. The colour becomes darker and the eggs become atritic. Atritic eggs are easily identified as they are small, hard and white. Ovaries in the later stages of eggs reabsorption have few new oocytes. The remnants of the old eggs collect in the middle of the organ. New oocytes production is restricted to the periphery of the ovary. Should you suspect this condition the ovaries should be preserved and stage verified by a qualified biologist. Occasionally, females have been observed which aborted spawning activity after they had became Ripe. Functionally speaking, eggs at this stage are no longer connected to the ovaries and cannot be reabsorbed. Instead they remain in the body cavity. Internal examination of a fish in this condition will show the newly developed gonad as well as residual (brown, desiccated) eggs which could not be reabsorbed in the posterior portion of the body cavity.

RESTING (RS): Fish in this category are sexually mature adults which have spawned in one or more previous spawning seasons but will not spawn in the coming spawning season. These fish are different from Reabsorbing fish in that their gonads are either not developing or are developing too slowly to be ready for the upcoming spawning season. This is a common condition for fish which do not spawn every year (alternate year spawners).

Male: This condition is extremely rare in males. It can only be used as an alternative to the Green category. A few cases of males in the resting condition have been observed. They are most common in northern latitudes where the growing season is short or in ultra-oligotrophic lakes. Testes will appear flaccid and dirty-white to yellow in colour. They will be larger in size than the testes of immature fish. A good indication is the size of the testicular artery in relation to the organ. In immature fish this artery is very thin whereas in resting males the testicular artery is much larger because of prior testicular development. Should you suspect this condition the testes should be preserved and stage verified by a qualified biologist.

Female: This condition is primarily observed in females but is still relatively infrequent, affecting usually only 0.5 to 1% of the population. This stage can only be used as an alternative to the Green category. It is most common in northern latitudes where the growing season is short or in ultra-oligotrophic lakes. The ovaries will appear to have some oocytes but they will be few in number and arrested in their development. The colour of resting ovaries varies greatly with fish species but most often they are a light orange. They will be larger in size than the ovaries of immature fish. A good indication is the size of the ovarian artery in relation to the organ. In immature fish this artery is very thin whereas in resting females the ovarian artery is much larger because of prior egg development. Should you suspect this condition the ovaries should be preserved and stage verified by a qualified biologist.

Appendix V.3 Fish Community Composition at Each Sampling Location

Table V.1 Fish Species Caught and Observed During Collections of White Sucker from Study Lakes, Moira River System, Fall 1999

Species Common Name	Scientific Name	Study Lakes
Species Common Name	Scientific Name	Consecon	Round	Moira	Stoco	Bend Bay
Largemouth bass	Micropterus salmoides		X	X		X
Smallmouth bass	Micropterus dolomieui		X	X	X	X
Rock bass	Ambloplites rupsetris	X			X	X
Yellow perch	Perca flavescens	X	X	X	X	X
Walleye	Stizostedion vitreum	X	X	X	X
Northern pike	Esox lucius	X	X	X	X	X
Muskellunge	Esox masquinongy		X	X	X
Pumpkinseed sunfish	Lepomis gibbosus	X
unknown sunfish sp.	Lepomis sp.		X	X
White sucker	Catostomus commersoni	X	X	X	X	X
Shorthead redhorse	Moxostoma macrolepidotum	X		X	X	X
Common carp	Cyprinus carpio	X
Brown bullhead	Ameiurus nebulosus	X				X
Longnose gar	Lepisosteus osseus	X			X

Table V.2 Fish Species Caught and Observed During Collections of Longnose Dace from River Study Sites, Moira River System, Fall 1999

Species Common Name	Scientific Name	River Study Sites
Species Common Name	Scientific Name	F-1	F-2	F-3
Rock bass	Ambloplites rupestris	X	X	X
Bluegill sunfish	Lepomis macrochirus		X
unknown sunfish sp.	Lepomis sp.	X
Longnose dace	Rhinichthys cateractae	X	X	X
Fall fish	Semotilus corporalis		X	X
Creek chub	Semotilus atromaculatus	X	X	X
Johnny darter	Etheostoma nigrum	X	X	X

Appendix V.4 Sentinel Fish Species Data

SENTINEL FISH SPECIES DATA

Sex:

F = female
M = male
U = unknown

Species:

WHSC = white sucker
LNDC = longnose dace

Maturity Stage:

SD = seasonal development
MA = maturing
IM = immature
U = unknown

Longnose Dace Sites:

F-1 = reference site upstream of Malone
F-2 = reference site at Malone
F-3 = exposure site downstream of Deloro Mine

Date	Fish #	Waterbody	Site	Species	Biomarker #	Fork Length (mm)	Total Length (mm)	Total Weight (g)	Carcass Weight (g)	Sex	Maturity Stage	Age	Liver Weight (g)	Gonad Weight (g)	Fecundity (# eggs)	Egg Diameter (mm)	% of Stomach Filled	Stomach Contents
Oct-99	2	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC002	483	512	1665	1432	F	SD	9	20.3	90.8	72331	1.09	0
Oct-99	1	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC001	491	523	1630	1321	M	SD	18	11.5	121.4			0
Oct-99	3	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC003	521	562	2081	1802	F	SD	12	25.6	114.3	77835	1.14	0
Oct-99	4	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC004	473	504	1446	1192	F	SD	15	20.4	83.1	55400	1.04	0
Oct-99	5	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC005	364	389	794	660	M	SD	5	8.5	62.4			0
Oct-99	6	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC006	355	377	691	580	M	SD	5	8	41.6			0
Oct-99	7	Consecon Lake	CL1	WHSC		280		340		M	IM	2
Oct-99	8	Consecon Lake	CL1	WHSC		274		255		U	IM	4
Oct-99	9	Consecon Lake	CL1	WHSC		253		216		U	IM	2
Oct-99	10	Consecon Lake	CL1	WHSC		198		118		U	IM	2
Oct-99	11	Consecon Lake	CL1	WHSC		166		60		U	IM	1
Oct-99	12	Consecon Lake	CL1	WHSC		155		52		U	IM
Oct-99	13	Stoco Lake	SL1	WHSC	MOE99FSL1WHSC013	367	392	707	575	M	SD	7	10.5	59.1			10	mush
Oct-99	14	Stoco Lake	SL1	WHSC	MOE99FSL1WHSC014	309	332	452	372	M	SD	4	5.2	36			0
Oct-99	15	Stoco Lake	SL1	WHSC	MOE99FSL1WHSC015	324	346	405	359	M	MA	6	5	5.9			0
Oct-99	16	Stoco Lake	SL1	WHSC	MOE99FSL1WHSC016	328	351	498	411	M	SD	7	5.7	34.5			0
Oct-99	17	Stoco Lake	SL1	WHSC	MOE99FSL1WHSC017	258	280	238	199	M	SD	6	2	13.7			10	black mush
Oct-99	18	Stoco Lake	SL1	WHSC		233		169		M	IM	3
Oct-99	19	Stoco Lake	SL1	WHSC	MOE99FSL1WHSC019	295	317	354	294	M	SD	8	3.4	21.8			0
Oct-99	20	Stoco Lake	SL1	WHSC	MOE99FSL1WHSC020	392	496	815	670	F	SD	13	12.1	39.3	31074	11.4	0
Oct-99	21	Stoco Lake	SL1	WHSC		169		60		U	IM	2
Oct-99	22	Stoco Lake	SL1	WHSC		164		49		U	IM	2
Oct-99	23	Stoco Lake	SL1	WHSC		282		280		M	IM
Oct-99	24	Stoco Lake	SL1	WHSC		170		61		U	UN
Oct-99	25	Stoco Lake	SL1	WHSC		231		169		U	UN
Oct-99	26	Stoco Lake	SL1	WHSC		212		114		U	UN
Oct-99	27	Stoco Lake	SL1	WHSC		211		130		U	UN
Oct-99	28	Stoco Lake	SL1	WHSC		235		159		U	UN
Oct-99	29	Stoco Lake	SL1	WHSC		186		80		U	UN
Oct-99	30	Moira River	F-2	LNDC	MOE99FMR2LNDC030	73	78	4.083	3.329	F	RB	2	0.048	0.302	1394	0.65	0
Oct-99	31	Moira River	F-2	LNDC	MOE99FMR2LNDC031	80	87	5.475	5.04	M	SD	2	0.039	0.072			0
Oct-99	32	Moira River	F-2	LNDC	MOE99FMR2LNDC032	70	76	3.839	3.263	F	SD	1	0.056	0.269	1257	0.62	0
Oct-99	33	Moira River	F-2	LNDC	MOE99FMR2LNDC033	85	91	5.793	4.926	F	SD	2	0.062	0.353	1161	0.67	0
Oct-99	34	Moira River	F-2	LNDC	MOE99FMR2LNDC034	71	76	4.239	3.718	M	SD	2	0.06	0.088			0
Oct-99	35	Moira River	F-2	LNDC	MOE99FMR2LNDC035	70	74	3.602	2.932	F	SD	1	0.064	0.286	1087	0.63	0
Oct-99	36	Moira River	F-2	LNDC	MOE99FMR2LNDC036	71	76	3.512	2.956	F	SD	1	0.035	0.189	1055	0.58	0
Oct-99	37	Moira River	F-2	LNDC	MOE99FMR2LNDC037	71	76	3.667	3.277	M	SD	3	0.029	0.047			0
Oct-99	38	Moira River	F-2	LNDC	MOE99FMR2LNDC038	71	77	3.854	3.412	M	SD	1	0.039	0.046			0
Oct-99	39	Moira River	F-2	LNDC	MOE99FMR2LNDC039	66	72	3.509	2.909	M	SD	3	0.072	0.05			0
Oct-99	40	Moira River	F-2	LNDC		51				U	UN
Oct-99	41	Moira River	F-2	LNDC		54				U	UN
Oct-99	42	Moira River	F-2	LNDC		45				U	UN
Oct-99	43	Moira River	F-2	LNDC		42				U	UN
Oct-99	44	Moira River	F-2	LNDC		44				U	UN
Oct-99	45	Moira River	F-2	LNDC		49				U	UN
Oct-99	46	Moira River	F-2	LNDC		53				U	UN
Oct-99	47	Moira River	F-2	LNDC		46				U	UN
Oct-99	48	Moira River	F-2	LNDC		43				U	UN
Oct-99	49	Moira River	F-2	LNDC		43				U	UN
Oct-99	50	Moira River	F-2	LNDC		63				U	UN
Oct-99	51	Moira River	F-2	LNDC		42				U	UN
Oct-99	52	Moira River	F-2	LNDC		45				U	UN
Oct-99	53	Moira River	F-2	LNDC		62				U	UN
Oct-99	54	Moira River	F-2	LNDC		43				U	UN
Oct-99	55	Moira River	F-2	LNDC		41				U	UN
Oct-99	56	Moira River	F-2	LNDC		43				U	UN
Oct-99	57	Moira River	F-2	LNDC		47				U	UN
Oct-99	58	Moira River	F-2	LNDC		42				U	UN
Oct-99	59	Moira River	F-2	LNDC		44				U	UN
Oct-99	60	Moira River	F-1	LNDC		47				U	IM
Oct-99	61	Moira River	F-1	LNDC		38				U	IM
Oct-99	62	Moira River	F-1	LNDC		47				U	IM
Oct-99	63	Moira River	F-1	LNDC		39				U	IM
Oct-99	64	Moira River	F-1	LNDC		48				U	IM
Oct-99	65	Moira River	F-1	LNDC		44				U	IM
Oct-99	66	Moira River	F-1	LNDC		43				U	IM
Oct-99	67	Moira River	F-1	LNDC		45				U	IM
Oct-99	68	Moira River	F-1	LNDC	MOE99FMR1LNDC068	79	84	5.672	4.741	F	SD	4	0.096	0.373	1838	0.59	0
Oct-99	69	Moira River	F-1	LNDC	MOE99FMR1LNDC069	75	80	4.523	3.824	F	SD	1	0.061	0.269	1295	0.62	0
Oct-99	70	Moira River	F-1	LNDC	MOE99FMR1LNDC070	79	85	5.428	4.398	F	SD	2	0.085	0.471	1733	0.63	25	unidentified
Oct-99	71	Moira River	F-1	LNDC	MOE99FMR1LNDC071	79	85	5.386	4.417	F	SD	2	0.09	0.47	2307	0.58	25	unidentified
Oct-99	72	Moira River	F-1	LNDC	MOE99FMR1LNDC072	67	72	3.316	2.8	F	SD	1	0.035	0.223	1017	0.62	0
Oct-99	73	Moira River	F-1	LNDC		51		1.431		U	IM
Oct-99	74	Moira River	F-1	LNDC		49		1.3		U	IM
Oct-99	75	Moira River	F-1	LNDC	MOE99FMR1LNDC075	66	70	3.305	2.79	F	SD	1	0.048	0.155	724	0.58	0
Oct-99	76	Moira River	F-1	LNDC	MOE99FMR1LNDC076	63	67	2.61	2.211	F	SD	1	0.028	0.124	562	0.64	0
Oct-99	77	Moira River	F-1	LNDC	MOE99FMR1LNDC077	63	68	3.065	2.604	F	SD	1	0.033	0.191	1005	0.63	0
Oct-99	78	Moira River	F-1	LNDC	MOE99FMR1LNDC078	78	82	5.19	4.369	F	SD	2	0.066	0.37	1602	0.62	0
Oct-99	79	Moira River	F-1	LNDC	MOE99FMR1LNDC079	65	73	3.079	2.58	F	SD	3	0.037	0.221	977	0.68	0
Oct-99	80	Moira River	F-2	LNDC		47				U	IM
Oct-99	81	Moira River	F-2	LNDC		44				U	IM
Oct-99	82	Moira River	F-2	LNDC		43				U	IM
Oct-99	83	Moira River	F-2	LNDC		45				U	IM
Oct-99	84	Moira River	F-2	LNDC		39				U	IM
Oct-99	85	Moira River	F-2	LNDC		49				U	IM
Oct-99	86	Moira River	F-2	LNDC		44				U	IM
Oct-99	87	Moira River	F-2	LNDC		43				U	IM
Oct-99	88	Moira River	F-2	LNDC		47				U	IM
Oct-99	89	Moira River	F-2	LNDC		38				U	IM
Oct-99	90	Moira River	F-2	LNDC		45				U	IM
Oct-99	91	Moira River	F-2	LNDC		46				U	IM
Oct-99	92	Moira River	F-2	LNDC		44				U	IM
Oct-99	93	Moira River	F-2	LNDC		48				U	IM
Oct-99	94	Moira River	F-2	LNDC		47				U	IM
Oct-99	95	Moira River	F-2	LNDC		44				U	IM
Oct-99	96	Moira River	F-2	LNDC	MOE99FMR2LNDC096	99	107	10.634	8.95	F	SD	4	0.123	0.8	2582	0.69	0
Oct-99	97	Moira River	F-2	LNDC	MOE99FMR2LNDC097	104	110	12.227	9.805	F	SD	5	0.261	1.135	3363	0.73	0
Oct-99	98	Moira River	F-2	LNDC	MOE99FMR2LNDC098	88	94	6.822	5.819	F	SD	3	0.067	0.363	1799	0.6	0
Oct-99	99	Moira River	F-2	LNDC	MOE99FMR2LNDC099	94	100	7.993	6.674	F	SD	5	0.088	0.536	2016	0.69	0
Oct-99	100	Moira River	F-2	LNDC	MOE99FMR2LNDC100	87	93	7.848	6.182	F	SD	1	0.129	0.605			100	mush
Oct-99	101	Moira River	F-2	LNDC	MOE99FMR2LNDC101	64	70	2.75	2.301	F	SD	2	0.037	0.135	712	0.58	0
Oct-99	102	Moira River	F-2	LNDC	MOE99FMR2LNDC102	51	55	1.376	1.152	M	SD	1	0.028	0.008			25	black mush
Oct-99	103	Moira River	F-2	LNDC	MOE99FMR2LNDC103	56	60	1.892	1.66	M	SD	0	0.018	0.022			100	black mush, 1 gastropod
Oct-99	104	Moira River	F-2	LNDC		53		1.6		U	IM
Oct-99	105	Moira River	F-2	LNDC	MOE99FMR2LNDC105	74	79	4.436	3.976	M	SD	2	0.071	0.072			0
Oct-99	106	Moira River	F-2	LNDC	MOE99FMR2LNDC106	71	77	3.794	3.323	M	SD	2	0.029	0.059			0
Oct-99	107	Moira River	F-2	LNDC	MOE99FMR2LNDC107	76	82	4.233	3.571	F	SD	2	0.065	0.267	1085	0.63	0
Oct-99	108	Moira River	F-2	LNDC	MOE99FMR2LNDC108	59	62	2.244	1.985	M	SD	2	0.017	0.027			30	black mush
Oct-99	109	Moira River	F-2	LNDC	MOE99FMR2LNDC109	73	78	3.875	3.221	F	SD	1	0.061	0.298	1669	0.6	0
Oct-99	110	Moira River	F-2	LNDC	MOE99FMR2LNDC110	65	70	2.823	2.327	F	SD	1	0.042	0.174	1166	0.63	25	black mush
Oct-99	111	Moira River	F-2	LNDC	MOE99FMR2LNDC111	73	79	3.674	3.088	F	SD	1	0.027	0.206	1140	0.63	0
Oct-99	112	Moira River	F-2	LNDC	MOE99FMR2LNDC112	70	75	3.184	2.718	F	SD	1	0.037	0.098	531	0.56	25	black mush
Oct-99	113	Moira River	F-2	LNDC	MOE99FMR2LNDC113	72	77	3.668	3.314	M	SD	1	0.034	0.041			0
Oct-99	114	Moira River	F-2	LNDC	MOE99FMR2LNDC114	53		1.466	1.309	M	SD	0	0.021	0.009			0
Oct-99	115	Moira River	F-2	LNDC	MOE99FMR2LNDC115	67	71	3.302	2.96	M	SD	2	0.036	0.042			0
Oct-99	116	Moira River	F-2	LNDC	MOE99FMR2LNDC116	72	77	3.979	3.159	F	SD	1	0.084	0.247	1004	0.62	25	black mush
Oct-99	117	Moira River	F-2	LNDC		72		3.878		U	UN	2
Oct-99	118	Moira River	F-2	LNDC		81		5.493		U	UN	1
Oct-99	119	Moira River	F-2	LNDC		91		7.655		U	UN	2
Oct-99	120	Moira River	F-2	LNDC		79		4.958		U	UN	2
Oct-99	121	Moira River	F-2	LNDC		86		6.974		U	UN	2
Oct-99	122	Moira River	F-1	LNDC		50				U	IM
Oct-99	123	Moira River	F-1	LNDC		46				U	IM
Oct-99	124	Moira River	F-1	LNDC		42				U	IM
Oct-99	125	Moira River	F-1	LNDC		49				U	IM
Oct-99	126	Moira River	F-1	LNDC		43				U	IM
Oct-99	127	Moira River	F-1	LNDC		51				U	IM
Oct-99	128	Moira River	F-1	LNDC		42				U	IM
Oct-99	129	Moira River	F-1	LNDC		44				U	IM
Oct-99	130	Moira River	F-1	LNDC		52				U	IM
Oct-99	131	Moira River	F-1	LNDC		41				U	IM
Oct-99	132	Moira River	F-1	LNDC		42				U	IM
Oct-99	133	Moira River	F-1	LNDC		47				U	IM
Oct-99	134	Moira River	F-1	LNDC		52				U	IM
Oct-99	135	Moira River	F-1	LNDC		47				U	IM
Oct-99	136	Moira River	F-1	LNDC		44				U	IM
Oct-99	137	Moira River	F-1	LNDC	MOE99FMR1LNDC137	66	71	3.093	2.5	F	SD	1	0.069	0.197	661	0.72	100	unknown black contents
Oct-99	138	Moira River	F-1	LNDC	MOE99FMR1LNDC138	64	68	2.835	2.491	M	SD	1	0.034	0.041			0
Oct-99	139	Moira River	F-1	LNDC	MOE99FMR1LNDC139	64	68	2.996	2.483	F	SD	1	0.06	0.209	721	0.65	0
Oct-99	140	Moira River	F-1	LNDC	MOE99FMR1LNDC140	68	73	3.395	2.782	F	SD	1	0.066	0.188	906	0.64	50	black mush
Oct-99	141	Moira River	F-1	LNDC	MOE99FMR1LNDC141	65	70	3.239	2.837	M	SD	1	0.045	0.063			100	black mush
Oct-99	142	Moira River	F-1	LNDC	MOE99FMR1LNDC142	61	65	2.716	2.19	F	SD	1	0.066	0.143	558	0.61	100	black mush
Oct-99	143	Moira River	F-1	LNDC	MOE99FMR1LNDC143	57	61	2.28	1.914	M	SD	2	0.036	0.032			50	black mush
Oct-99	144	Moira River	F-1	LNDC	MOE99FMR1LNDC144	65	69	2.552	2.204	M	SD	2	0.029	0.039			100	black mush
Oct-99	145	Moira River	F-1	LNDC	MOE99FMR1LNDC145	65	69	3.147	2.582	F	SD	1	0.051	0.129	711	0.51	100	black mush
Oct-99	146	Moira Moira River	F-1	LNDC	MOE99FMR1LNDC146	67	72	3.129	2.73	M	SD	1	0.046	0.045			30	black mush
Oct-99	147	Moira River	F-1	LNDC	MOE99FMR1LNDC147	62	67	2.418	2.018	F	SD	3	0.032	0.153	689	0.65	0
Oct-99	148	Moira River	F-1	LNDC	MOE99FMR1LNDC148	62	66	2.767	2.444	M	SD	4	0.043	0.045			0
Oct-99	149	Moira River	F-1	LNDC	MOE99FMR1LNDC149	65	70	3.33	2.828	M	SD	2	0.058	0.051			50	black mush
Oct-99	150	Moira River	F-1	LNDC	MOE99FMR1LNDC150	61	65	2.405	2.01	F	SD	1	0.04	0.163	696	0.57	100	black mush
Oct-99	151	Moira River	F-1	LNDC	MOE99FMR1LNDC151	67	72	3.555	2.982	F	SD	2	0.054	0.219	1005	0.63	30	black mush
Oct-99	152	Moira River	F-1	LNDC	MOE99FMR1LNDC152	66	71	3.045	2.513	F	SD	3	0.058	0.211	766	0.62	50	black mush
Oct-99	153	Moira River	F-1	LNDC	MOE99FMR1LNDC153	64	68	2.931	2.515	F	SD	1	0.058	0.119			0
Oct-99	154	Moira River	F-1	LNDC	MOE99FMR1LNDC154	63	68	2.807	2.475	M	SD	3	0.044	0.038			50	black mush
Oct-99	155	Moira River	F-1	LNDC	MOE99FMR1LNDC155	67	72	3.457	3.009	M	SD	2	0.057	0.059			30	black mush
Oct-99	156	Moira River	F-1	LNDC	MOE99FMR1LNDC156	75	81	4.785	4.155	M	SD	3	0.07	0.08			0
Oct-99	157	Moira River	F-1	LNDC	MOE99FMR1LNDC157	67	72	3.511	2.882	F	SD	2	0.063	0.191	1118	0.57	50	black mush
Oct-99	158	Moira River	F-1	LNDC	MOE99FMR1LNDC158	60	65	2.355	1.989	F	SD	1	0.036	0.081	507	0.62	0
Oct-99	159	Moira River	F-1	LNDC	MOE99FMR1LNDC159	66	70	3.138	2.646	F	SD	1	0.052	0.156			10	black mush
Oct-99	160	Moira River	F-1	LNDC	MOE99FMR1LNDC160	69	75	3.649	2.985	F	SD	2	0.059	0.252	1163	0.6	50	black mush
Oct-99	161	Moira River	F-1	LNDC	MOE99FMR1LNDC161	72	78	4.576	4.064	M	SD	2	0.064	0.063			10	black mush
Oct-99	162	Moira River	F-1	LNDC		98		7.687		U	UN	1
Oct-99	163	Moira River	F-1	LNDC		82		5.69		U	UN	1
Oct-99	164	Moira River	F-1	LNDC		77		4.752		U	UN	1
Oct-99	165	Moira River	F-1	LNDC		75		5.421		U	UN	1
Oct-99	166	Moira River	F-1	LNDC		75		4.84		U	UN	2
Oct-99	167	Moira River	F-1	LNDC		71		4.234		U	UN	1
Oct-99	168	Moira River	F-1	LNDC		75		4.368		U	UN	2
Oct-99	169	Moira River	F-1	LNDC		72		3.937		U	UN	1
Oct-99	170	Moira River	F-1	LNDC		70		3.423		U	UN	2
Oct-99	171	Moira River	F-1	LNDC		68		3.398		U	UN	1
Oct-99	172	Moira River	F-1	LNDC		45				U	IM
Oct-99	173	Moira River	F-1	LNDC		48				U	IM
Oct-99	174	Moira River	F-1	LNDC		43				U	IM
Oct-99	175	Moira River	F-1	LNDC		46				U	IM
Oct-99	176	Moira River	F-1	LNDC		51				U	IM
Oct-99	177	Moira River	F-1	LNDC		43				U	IM
Oct-99	178	Moira River	F-1	LNDC		48				U	IM
Oct-99	179	Moira River	F-1	LNDC		46				U	IM
Oct-99	180	Moira River	F-1	LNDC		49				U	IM
Oct-99	181	Moira River	F-1	LNDC	MOE99FMR1LNDC181	62	66	2.563	2.278	M	SD	2	0.053	0.032			0
Oct-99	182	Moira River	F-1	LNDC	MOE99FMR1LNDC182	61	65	2.482	2.025	F	SD	1	0.051	0.158	741	0.57	100	black mush
Oct-99	183	Moira River	F-1	LNDC	MOE99FMR1LNDC183	65	70	3.075	2.736	M	SD	3	0.041	0.041			50	black mush
Oct-99	184	Moira River	F-1	LNDC	MOE99FMR1LNDC184	79	85	5.281	4.633	M	SD	4	0.055	0.095			25	black mush
Oct-99	185	Moira River	F-1	LNDC	MOE99FMR1LNDC185	75	80	4.582	4.113	M	SD	3	0.054	0.054			0
Oct-99	186	Moira River	F-1	LNDC		84		7.2		F	SD
Oct-99	187	Moira River	F-1	LNDC		84		6.3		F	SD
Oct-99	188	Moira River	F-2	LNDC		76				U	UN
Oct-99	189	Moira River	F-2	LNDC		76				U	UN
Oct-99	190	Moira River	F-2	LNDC		45				U	IM
Oct-99	191	Moira River	F-2	LNDC		45				U	IM
Oct-99	192	Moira River	F-2	LNDC		73				U	UN
Oct-99	193	Moira River	F-2	LNDC		53				U	IM
Oct-99	194	Moira River	F-2	LNDC		50				U	IM
Oct-99	195	Moira River	F-2	LNDC		70				U	UN
Oct-99	196	Moira River	F-2	LNDC		75				U	IM
Oct-99	197	Moira River	F-2	LNDC		72				U	UN
Oct-99	198	Moira River	F-2	LNDC		42				U	IM
Oct-99	199	Moira River	F-2	LNDC		48				U	IM
Oct-99	200	Moira River	F-2	LNDC		48				U	IM
Oct-99	201	Moira River	F-2	LNDC		73				U	UN
Oct-99	202	Moira River	F-2	LNDC		74				U	UN
Oct-99	203	Moira River	F-2	LNDC		48				U	IM
Oct-99	204	Moira River	F-2	LNDC		71				U	UN
Oct-99	205	Moira River	F-2	LNDC		76				U	UN
Oct-99	206	Moira River	F-2	LNDC		42				U	IM
Oct-99	207	Moira River	F-2	LNDC		75				U	UN
Oct-99	208	Moira River	F-2	LNDC		77				U	UN
Oct-99	209	Moira River	F-2	LNDC		51				U	IM
Oct-99	210	Moira River	F-2	LNDC		45				U	IM
Oct-99	211	Moira River	F-2	LNDC		46				U	IM
Oct-99	212	Moira River	F-2	LNDC		47				U	IM
Oct-99	213	Moira River	F-2	LNDC		48				U	IM
Oct-99	214	Moira River	F-2	LNDC		45				U	IM
Oct-99	215	Moira River	F-2	LNDC		50				U	IM
Oct-99	216	Moira River	F-2	LNDC		45				U	IM
Oct-99	217	Moira River	F-2	LNDC		44				U	IM
Oct-99	218	Moira River	F-2	LNDC		45				U	IM
Oct-99	219	Moira River	F-2	LNDC		42				U	IM
Oct-99	220	Moira River	F-2	LNDC		42				U	IM
Oct-99	221	Moira River	F-2	LNDC	MOE99FMR2LNDC221	56	61	1.745	1.558	M	SD	1	0.011	0.019			0
Oct-99	222	Moira River	F-2	LNDC	MOE99FMR2LNDC222	68	73	3.514	2.935	F	SD	1	.0.56	0.195	868	0.61	100	black mush
Oct-99	223	Moira River	F-2	LNDC	MOE99FMR2LNDC223	71	76	3.767	3.353	M	SD	3	0.048	0.05			0
Oct-99	224	Moira River	F-2	LNDC	MOE99FMR2LNDC224	56	60	1.598	1.396	M	SD	2	0.016	0.015			0
Oct-99	225	Moira River	F-2	LNDC	MOE99FMR2LNDC225	68	73	3.104	2.674	F	SD	1	0.048	0.154	575	0.7	0
Oct-99	226	Moira River	F-2	LNDC	MOE99FMR2LNDC226	54	58	1.446	1.253	M	SD	0	0.014				0
Oct-99	227	Moira River	F-2	LNDC	MOE99FMR2LNDC227	76	81	3.858	3.448	M	SD	2	0.061	0.058
Oct-99	228	Moira River	F-2	LNDC	MOE99FMR2LNDC228	75	80	4.377	3.716	F	SD	2	0.081	0.311	1399	0.61	0
Oct-99	229	Moira River	F-2	LNDC	MOE99FMR2LNDC229	73	78	3.57	3.067	M	SD	2	0.039	0.042			25	black mush
Oct-99	230	Moira River	F-2	LNDC	MOE99FMR2LNDC230	79	84	4.986	4.513	M	SD	2	0.06	0.051			0
Oct-99	231	Moira River	F-2	LNDC	MOE99FMR2LNDC229	102		11.091		U	UN	2
Oct-99	232	Moira River	F-2	LNDC	MOE99FMR2LNDC230	99		9.782		U	UN	3
Oct-99	233	Moira River	F-2	LNDC		94		9		U	UN	2
Oct-99	234	Moira River	F-2	LNDC		92		7.882		U	UN	1
Oct-99	235	Moira River	F-2	LNDC		79		4.982		U	UN	1
Oct-99	236	Moira River	F-2	LNDC		72		4.341		U	UN
Oct-99	237	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC237	420	447	1100	920	F	SD	4	15.9	69.6	57069	1.11	20	chyme
Oct-99	238	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC238	410	438	1079	929	F	SD	5	13.8	64.9	50032	1.16	20	chyme
Oct-99	239	Consecon Lake	CL1	WHSC		310		380		M	MA
Oct-99	240	Consecon Lake	CL1	WHSC		294		361		U	IM
Oct-99	241	Consecon Lake	CL1	WHSC		270		285		U	IM
Oct-99	242	Consecon Lake	CL1	WHSC		295		340		U	IM
Oct-99	243	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC243	395	414	949	795	F	SD	6	13.3	59.8	35681	1.4	5	black mush
Oct-99	244	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC244	494	530	2011	1669	F	SD	15	30.1	139.8	87264	1.15	0
Oct-99	245	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC245	381	450	925	790	F	SD	6	15.8	44	35210	0.93	0
Oct-99	246	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC246	350	372	639	521	M	SD	6	6	56.9			10	black mush
Oct-99	247	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC247	435	464	1321	1079	M	SD	6	15	133.3			0
Oct-99	248	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC248	415	440	1120	942	F	SD	6	15.2	65	48575	1.14	0
Oct-99	249	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC249	445	473	1351	1135	M	SD	10	13.4	108.4			0
Oct-99	250	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC250	439	468	1231	1060	F	SD	7	14.8	58.6	39686	1.2	0
Oct-99	251	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC251	435	468	1281	1065	F	SD	6	18.7	89	57605	1.17	50	black mush
Oct-99	252	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC252	408	435	1020	849	M	SD		5	11.5	86.7			0
Oct-99	253	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC253	341	365	619	524	F	SD	6	7.3	33.5	23914	1.21	0
Oct-99	254	Consecon Lake	CL1	WHSC						U	UN
Oct-99	255	Stoco Lake	SL1	WHSC	MOE99FSL1WHSC255	282	295	270		M	SD	8	2.8	13.9			0
Oct-99	256	Stoco Lake	SL1	WHSC		278		300		U	IM
Oct-99	257	Stoco Lake	SL1	WHSC		228		160		U	IM
Oct-99	258	Stoco Lake	SL1	WHSC		270		280		U	IM
Oct-99	259	Stoco Lake	SL1	WHSC	MOE99FSL1WHSC259	283	300	320	270	M	SD	2	3.1	19.9			0
Oct-99	260	Stoco Lake	SL1	WHSC		285		309		U	IM
Oct-99	261	Stoco Lake	SL1	WHSC	MOE99FSL1WHSC262	236		190		U	IM
Oct-99	262	Stoco Lake	SL1	WHSC	MOE99FSL1WHSC263	376	398	820	617	F	SD	10	14.6	45.1	32284	1.16	20	black mush
Oct-99	263	Stoco Lake	SL1	WHSC	MOE99FSL1WHSC264	340	365	630	530	F	SD	5	11.4	38.3	27362	1.25	100	green mush
Oct-99	264	Stoco Lake	SL1	WHSC		291		345		U	IM
Oct-99	265	Stoco Lake	SL1	WHSC		290		310		U	IM
Oct-99	266	Stoco Lake	SL1	WHSC		198		115		U	IM
Oct-99	267	Stoco Lake	SL1	WHSC		210		115		U	IM
Oct-99	268	Stoco Lake	SL1	WHSC	MOE99FML1WHSC268	374	399	727	595	M	SD	8	7.9	40.3			10	invert parts
Oct-99	269	Moira Lake	ML1	WHSC	MOE99FML1WHSC269	409	442	831	691	M	SD	12	8.5	64.7			0
Oct-99	270	Moira Lake	ML1	WHSC	MOE99FML1WHSC270	443	476	1149	950	F	SD	7	17.7	62	41437	1.19	0
Oct-99	271	Moira Lake	ML1	WHSC		426		1085		F	RS	8
Oct-99	272	Moira Lake	ML1	WHSC	MOE99FML1WHSC272	340	362	543	449	M	SD	5	5.5	34.5
Oct-99	273	Moira Lake	ML1	WHSC	MOE99FML1WHSC273	377	399	663	550	F	SD	12	8.4	34.5	30947	1.13	0
Oct-99	274	Moira Lake	ML1	WHSC	MOE99FML1WHSC274	363	385	690	580	F	SD	12	11.3	46.2	30875	1.131	0
Oct-99	275	Moira Lake	ML1	WHSC	MOE99FML1WHSC275	380	409	820	690	F	SD	9	14	55.5	36126	1.26	10	mollusk
Oct-99	276	Moira Lake	ML1	WHSC	MOE99FML1WHSC276	430	458	1250	1030	F	SD	11	22.5	87.7	43388	1.42	0
Oct-99	277	Moira Lake	ML1	WHSC	MOE99FML1WHSC277	381	410	860	750	F	SD	11	14.5	46.8	31343	1.22	0
Oct-99	278	Moira Lake	ML1	WHSC	MOE99FML1WHSC278	283	294	330	300	F	IM	3	5.3	2.2			0
Oct-99	279	Moira Lake	ML1	WHSC	MOE99FML1WHSC279	276	289	270	240	F	IM	4	303	1.1			20	chironomids
Oct-99	280	Moira Lake	ML1	WHSC	MOE99FML1WHSC280	418	447	1090	920	F	SD	7	16.1	70.1	47978	1.24	50
Oct-99	281	Moira Lake	ML1	WHSC	MOE99FML1WHSC281	406	427	980	820	F	SD	7	15.8	55.6	36635	1.18	0
Oct-99	282	Moira Lake	ML1	WHSC	MOE99FML1WHSC282	332	355	489	401	M	SD	7	4.9	37.8			0
Oct-99	283	Moira Lake	ML1	WHSC	MOE99FML1WHSC283	382	405	730	620	F	SD	9	13.3	35.6	25225	1.16	0
Oct-99	284	Moira Lake	ML1	WHSC	MOE99FML1WHSC284	344	367	539	455	M	SD	7	6.2	30.3			2
Oct-99	285	Moira Lake	ML1	WHSC	MOE99FML1WHSC285	398	422	970	785	M	SD	12	13.6	79.6				chyme
Oct-99	286	Moira Lake	ML1	WHSC	MOE99FML1WHSC286	418	442	1021	822	F	SD	13	18.7	64.5	34239	1.34	0
Oct-99	287	Moira Lake	ML1	WHSC	MOE99FML1WHSC287	372	395	690	560	F	SD	13	15.9	51.1	29106	1.29	10	chyme
Oct-99	288	Moira Lake	ML1	WHSC	MOE99FML1WHSC288	351	379	550	470	M	SD	9	4.9	25.5			0
Oct-99	289	Moira Lake	ML1	WHSC	MOE99FML1WHSC289	357	378	650	530	M	SD	12	8.3	33.9			0
Oct-99	290	Moira Lake	ML1	WHSC	MOE99FML1WHSC290	360	385	592	499	F	SD	14	9.8	31.4	22174	1.09	0
Oct-99	291	Moira Lake	ML1	WHSC	MOE99FML1WHSC291	403	428	870	730	F	SD	10	12.9	50	32725	1.24	0
Oct-99	292	Moira Lake	ML1	WHSC	MOE99FML1WHSC292	353	380	641	535	M	SD	10	5.3	39.3			0
Oct-99	293	Moira Lake	ML1	WHSC	MOE99FML1WHSC293	370	391	680	570	M	SD	10	7.5	54.4			0
Oct-99	294	Moira Lake	ML1	WHSC	MOE99FML1WHSC294	349	369	640	530	F	SD	9	11.9	38.2	22591	1.33	20	chyme
Oct-99	295	Moira Lake	ML1	WHSC		282		305		M	IM	6
Oct-99	296	Moira Lake	ML1	WHSC	MOE99FML1WHSC296	373	391	745	610	M	SD	8	7.4	48.7			0	chyme
Oct-99	297	Moira Lake	ML1	WHSC	MOE99FML1WHSC297	422	452	980	830	F	SD	12	13.3	65.6	47219	1.2	0
Oct-99	298	Moira Lake	ML1	WHSC	MOE99FML1WHSC298	384	409	780	660	M	SD	11	8.3	56.3			0	chyme
Oct-99	299	Moira Lake	ML1	WHSC	MOE99FML1WHSC299	371	400	752	532	F	SD	13	14.4	42	31707	1.2	5	unidentified
Oct-99	300	Round Lake	RL1	WHSC	MOE99FRLWHSC300	372	399	715	599	M	SD	10	8	42.3			0
Oct-99	301	Round Lake	RL1	WHSC	MOE99FRLWHSC301	319	342	421	359	M	SD	5	4.2	18.2			0
Oct-99	302	Round Lake	RL1	WHSC	MOE99FRL1WHSC302	321	342	390	335	F	SD	9	6.6	21	14540	1.23
Oct-99	303	Round Lake	RL1	WHSC		172		67		M	IM	2
Oct-99	304	Round Lake	RL1	WHSC		215		120		U	UN
Oct-99	305	Round Lake	RL1	WHSC		200		94		U	UN
Oct-99	306	Round Lake	RL1	WHSC		216		120		U	UN
Oct-99	307	Round Lake	RL1	WHSC		225		140		F	IM	3
Oct-99	308	Round Lake	RL1	WHSC		123		21.1		M	IM	1
Oct-99	309	Round Lake	RL1	WHSC	MOE99FRL1WHSC309	275	288	255	210	M	SD	9	2.6	14.2			0
Oct-99	310	Round Lake	RL1	WHSC	MOE99FRL1WHSC310	388	409	895	760	F	SD	9	11.8	45.4	28474	1.19	0
Oct-99	311	Round Lake	RL1	WHSC	MOE99FRL1WHSC311	323	343	440	360	F	SD	7	5.9	22.7	18706	1.07	0
Oct-99	312	Round Lake	RL1	WHSC	MOE99FRL1WHSC312	285	304	290	245	M	SD	8	2.8	11			0
Oct-99	313	Round Lake	RL1	WHSC	MOE99FRL1WHSC313	318	337	390	330	F	SD	10	6.2	16	12784	1.13	0
Oct-99	314	Round Lake	RL1	WHSC		238		170		F	IM
Oct-99	315	Round Lake	RL1	WHSC		236		160		U	IM
Oct-99	316	Round Lake	RL1	WHSC		228		170		U	IM
Oct-99	317	Round Lake	RL1	WHSC		239		170		U	IM
Oct-99	318	Round Lake	RL1	WHSC		171		70		U	IM
Oct-99	319	Round Lake	RL1	WHSC		139		50		U	IM
Oct-99	320	Round Lake	RL1	WHSC		144		40		U	IM
Oct-99	321	Round Lake	RL1	WHSC		223		140		U	IM
Oct-99	322	Round Lake	RL1	WHSC	MOE99FRL1WHSC322	322	341	500	425	F	SD	9	9.7	23.3	12639	1.2	0
Oct-99	323	Round Lake	RL1	WHSC	MOE99FRL1WHSC323	313	331	380	330	F	SD	8	6.3	15.5	10087	1.18	0
Oct-99	324	Moira River	MR4	WHSC	MOE99FMR4WHSC324	420	455	1020	830	F	SD	13	20	65.8	45982	1.22	0
Oct-99	325	Moira River	MR4	WHSC	MOE99FMR4WHSC325	355	373	640	550	M	SD	9	7.2	38.8			0
Oct-99	326	Moira River	MR4	WHSC	MOE99FMR4WHSC326	386	406	780	670	F	SD	10	16	46.3	27058	1.3	0
Oct-99	327	Moira River	MR4	WHSC	MOE99FMR4WHSC327	386	409	900	750	F	SD	9	20.3	52.7	29480	1.29	0
Oct-99	328	Moira River	MR4	WHSC		374	401	730	600	M	SD	9	8.9	50.1			0
Oct-99	329	Moira River	MR4	WHSC		100		11.1		U	IM	0
Oct-99	330	Moira River	MR4	WHSC	MOE99FMR4WHSC330	356	375	600	510	M	SD	7	6.6	36.4			0
Oct-99	331	Moira River	MR4	WHSC		245		210		F	IM	5
Oct-99	332	Moira River	MR4	WHSC	MOE99FMR4WHSC332	335	351	520	450	M	SD	8	5.9	27.7			0
Oct-99	333	Moira River	MR4	WHSC	MOE99FMR4WHSC323	293	309	330	280	F	SD	7	5.4	16.1	13521	1.16	0
Oct-99	334	Moira River	MR4	WHSC		228		150		M	IM	4
Oct-99	335	Moira River	MR4	WHSC		187		80		M	IM	1
Oct-99	336	Moira Lake	ML1	WHSC	MOE99FML1WHSC336	350		630	540	M	SD	9	9.6	34.1			0
Oct-99	337	Moira Lake	ML1	WHSC	MOE99FML1WHSC337	406	437	906	739	F	SD	12	17.6	44.5	26935	1.31	0
Oct-99	338	Moira Lake	ML1	WHSC	MOE99FML1WHSC338	330	350	530	450	F	SD	6	8.1	26.2	21729	1.14	0
Oct-99	339	Moira Lake	ML1	WHSC	MOE99FML1WHSC339	406	439	1073	895	F	SD	11	17.7	69.5	37213	1.26	0
Oct-99	340	Moira Lake	ML1	WHSC	MOE99FML1WHSC340	376	400	790	660	M	SD	10	11.1	46.1			0
Oct-99	341	Moira Lake	ML1	WHSC	MOE99FML1WHSC341	366	394	790	652	M	SD	10	13.4	61.9			0
Oct-99	342	Moira Lake	ML1	WHSC	MOE99FML1WHSC342	423	450	1030	840	F	SD	12	14.7	72.7	37395	1.35	0
Oct-99	343	Moira Lake	ML1	WHSC	MOE99FML1WHSC343	377	407	782	648	M	SD	9	9.9	50.5			0
Oct-99	344	Moira Lake	ML1	WHSC	MOE99FML1WHSC344	348	372	580	490	M	SD	10	7.9	44.6			0
Oct-99	345	Moira Lake	ML1	WHSC	MOE99FML1WHSC345	365	388	730	595	F	SD	8	13.6	54.2	30001	1.33	0
Oct-99	346	Moira Lake	ML1	WHSC	MOE99FML1WHSC346	331	358	520	450	M	SD	5	4.2	29.7			0
Oct-99	347	Moira Lake	ML1	WHSC	MOE99FML1WHSC347	331	355	480	400	M	SD	7	5.1	32.6			0
Oct-99	348	Moira Lake	ML1	WHSC	MOE99FML1WHSC348	438	450	1100	900	F	SD	11	19.7	77.9	42739	1.36	0
Oct-99	349	Moira Lake	ML1	WHSC		265		260		F	IM	6
Oct-99	350	Moira Lake	ML1	WHSC		175		186		M	IM	3
Oct-99	351	Moira River	MR7	WHSC		415		910		F	SD	12
Oct-99	352	Moira River	MR7	WHSC		285		300		F	SD	5
Oct-99	353	Moira River	MR7	WHSC		233		170		F	IM	4
Oct-99	354	Moira River	MR7	WHSC		380		767		F	SD	7
Oct-99	355	Moira River	MR7	WHSC		203		115		F	SD	4
Oct-99	356	Moira River	MR7	WHSC		305		350		F	SD	7
Oct-99	357	Moira River	MR7	WHSC		182		80		M	SD	1
Oct-99	358	Moira River	MR7	WHSC		190		80		F	IM	4
Oct-99	359	Moira River	MR7	WHSC		230		160		U	IM	4
Oct-99	360	Moira River	MR7	WHSC		211		112		U	IM
Oct-99	361	Moira River	MR7	WHSC		234		152		M	IM	5
Oct-99	362	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC362	399	422	865	745	F	SD	6	8.2	43.8	32114	1.11	0
Oct-99	363	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC363	481	416	1628	1330	F	SD	8	25.7	124	58461	1.31	5	unidentified material
Oct-99	364	Consecon Lake	CL1	WHSC		302		380		M	IM
Oct-99	365	Consecon Lake	CL1	WHSC		193		135		U	IM
Oct-99	366	Consecon Lake	CL1	WHSC		215		160		U	IM
Oct-99	367	Consecon Lake	CL1	WHSC		235		195		U	IM
Oct-99	368	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC368	477	516	1470	1240	F	SD		23.7	63.4	47293	1.14	0
Oct-99	369	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC368	480	501	1530	1230	M	SD	14	18.2	141			0
Oct-99	370	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC368	573	605	2500	2030	F	SD	15	41.1	113.6	60167	1.19	10	chyme
Oct-99	371	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC368	415	440	1090	890	M	SD	8	12.6	84.4			0
Oct-99	372	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC368	451	482	1270	1060	F	SD	8	13.1	77.8	51791	1.17	0
Oct-99	373	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC368	471	502	1890	1510	F	SD	10	32.7	157.2	85238	1.28	20	black mush
Oct-99	374	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC368	436	465	1350	1110	F	SD	7	12.4	97.7	58426	1.23	0
Oct-99	375	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC368	435	463	1370	1160	F	SD	11	18.6	71.7	47800	1.19	0
Oct-99	376	Consecon Lake	CL1	WHSC		316		430		F	IM
Oct-99	377	Consecon Lake	CL1	WHSC	MOE99FCL1WHSC377	350	374	650	560	F	SD	6	8.5	28.4	25310	1.06	0
Oct-99	378	Moira River	MR4	WHSC	MOE99FMR4WHSC378	385	412	769	661	F	SD	12	10.8	43	31169	1.2	0
Oct-99	379	Moira River	MR4	WHSC	MOE99FMR4WHSC379	392	420	820	710	F	SD	7	14.6	38.1	23955	1.21	0
Oct-99	380	Moira River	MR4	WHSC	MOE99FMR4WHSC380	392	420	892	761	F	SD	11	19.2	51	31911	1.3	0
Oct-99	381	Moira River	MR4	WHSC	MOE99FMR4WHSC381	404	433	819	680	F	SD	10	14.7	47.9	30915	1.22	0
Oct-99	382	Moira River	MR4	WHSC	MOE99FMR4WHSC382	360	382	681	575	M	SD	13	15.7	41.7			0
Oct-99	383	Moira River	MR4	WHSC	MOE99FMR4WHSC383	315	331	425	360	M	SD	10	7.7	22.8			0
Oct-99	384	Moira River	MR4	WHSC		214		109		U	IM
Oct-99	385	Moira River	MR4	WHSC		161		54		U	IM
Oct-99	386	Moira River	MR4	WHSC		124		26		U	IM
Oct-99	387	Moira River	MR4	WHSC		129		43		U	IM
Oct-99	388	Moira River	MR4	WHSC	MOE99FMR4WHSC388	360	385	610	510	M	SD	9	6.2	34.1			0
Oct-99	389	Moira River	MR4	WHSC	MOE99FMR4WHSC389	345	369	590	510	F	SD	7	8.8	31.3	21001	1.19	0
Oct-99	390	Moira River	MR4	WHSC	MOE99FMR4WHSC390	374	396	670	580	F	SD	9	12.1	38.6	27311	1.21	0
Oct-99	391	Moira River	MR4	WHSC	MOE99FMR4WHSC391	400	430	860	730	F	SD	8	12.8	49.2	31210	1.23	0
Oct-99	392	Moira River	MR4	WHSC	MOE99FMR4WHSC392	380	402	800	680	M	SD	11	9.9	43.1			0
Oct-99	393	Round Lake	RL1	WHSC	MOE99FRL1WHSC393	352	376	601	505	F	SD	6	8.8	29	19302	1.17	0
Oct-99	394	Round Lake	RL1	WHSC	MOE99FRL1WHSC394	357	380	619	535	M	SD	12	8.1	27.1			0
Oct-99	395	Round Lake	RL1	WHSC	MOE99FRL1WHSC395	305	326	369	315	F	SD	5	8.7	16.6	13283	1.13	0
Oct-99	396	Round Lake	RL1	WHSC		252		190		F	IM
Oct-99	397	Round Lake	RL1	WHSC		141		50		U	IM
Oct-99	398	Round Lake	RL1	WHSC		142		55		U	IM
Oct-99	399	Round Lake	RL1	WHSC		218		125		U	IM
Oct-99	400	Round Lake	RL1	WHSC		242		175		U	IM
Oct-99	401	Round Lake	RL1	WHSC		243		165		U	IM
Oct-99	402	Round Lake	RL1	WHSC		236		162		U	IM
Oct-99	403	Round Lake	RL1	WHSC		195		62		U	IM
Oct-99	404	Round Lake	RL1	WHSC		255		190		U	IM
Oct-99	405	Round Lake	RL1	WHSC	MOE99FRL1WHSC405	365	387	630	540	F	SD	10	3.7	31.2	18062	1.35	0
Oct-99	406	Round Lake	RL1	WHSC	MOE99FRL1WHSC406	347	369	600	490	F	SD	9	8.9	29.7	18314	1.17	0
Oct-99	407	Round Lake	RL1	WHSC	MOE99FRL1WHSC407	404	431	880	730	F	SD	11	15.6	57.2	33839	1.28	0
Oct-99	408	Round Lake	RL1	WHSC	MOE99FRL1WHSC408	338	362	540	440	M	SD	6	4.8	33.4			0
Oct-99	409	Round Lake	RL1	WHSC		259		160		U	IM
Oct-99	410	Round Lake	RL1	WHSC		247		140		U	IM
Oct-99	411	Round Lake	RL1	WHSC		211		110		U	IM
Oct-99	412	Round Lake	RL1	WHSC		183		80		U	IM
Oct-99	413	Round Lake	RL1	WHSC		180		80		U	IM
Oct-99	414	Round Lake	RL1	WHSC		215		130		U	IM
Oct-99	415	Round Lake	RL1	WHSC		215		130		U	IM
Oct-99	416	Round Lake	RL1	WHSC		182		60		U	IM
Oct-99	417	Round Lake	RL1	WHSC		159		50		U	IM
Oct-99	418	Round Lake	RL1	WHSC		155		50		U	IM
Oct-99	419	Round Lake	RL1	WHSC		145		40		U	IM
Oct-99	420	Round Lake	RL1	WHSC		153		60		U	IM
Oct-99	421	Round Lake	RL1	WHSC		166		80		U	IM
Oct-99	422	Round Lake	RL1	WHSC	MOE99FRL1WHSC422	265	283	260	210	M	SD	7	2.6	10.9			0
Oct-99	423	Round Lake	RL1	WHSC	MOE99FRL1WHSC423	298	313	330	280	F	SD	6	6.8	14.9	9851	1.25	0
Oct-99	424	Round Lake	RL1	WHSC	MOE99FRL1WHSC424	280	297	300	250	F	SD	6	6.7	16.4	9662	1.24	0
Oct-99	425	Round Lake	RL1	WHSC	MOE99FRL1WHSC425	273	287	250	210	F	SD	8	3.4	10.6	7611	1.07	0
Oct-99	426	Round Lake	RL1	WHSC		213		140		U	IM
Oct-99	427	Round Lake	RL1	WHSC	MOE99FRL1WHSC427	244	260	200	170	F	SD	3	2.7	8.1	6920	1.02	0
Oct-99	428	Round Lake	RL1	WHSC	MOE99FRL1WHSC428	333	362	520	450	F	SD	8	7.6	30.5	17679	1.3	0
Oct-99	429	Round Lake	RL1	WHSC		381		818		F	SD	7
Oct-99	430	Round Lake	RL1	WHSC		313		441		F	SD	4
Oct-99	431	Moira River	MR6	WHSC		375		719		M	SD	8
Oct-99	432	Moira River	MR6	WHSC		310		429		M	SD	4
Oct-99	433	Moira River	MR6	WHSC		239		170		M	IM	3
Oct-99	434	Moira River	MR6	WHSC		304		390		F	IM	5
Oct-99	435	Moira River	MR6	WHSC		254		203		F	IM	3
Oct-99	436	Moira River	MR6	WHSC		232		152		F	IM	4
Oct-99	437	Moira River	MR6	WHSC		221		149		M	IM	2
Oct-99	438	Moira River	MR6	WHSC		378		659		U	UN
Oct-99	439	Moira River	MR6	WHSC		360		621		U	UN
Oct-99	440	Moira River	MR6	WHSC		403		961		U	UN
Oct-99	441	Moira River	MR6	WHSC		151		32		U	UN
Oct-99	442	Moira River	MR5	WHSC		301		330		F	IM	2
Oct-99	443	Moira River	MR5	WHSC		275		280		F	SD	5
Oct-99	444	Moira River	MR5	WHSC		193		90		F	IM	3
Oct-99	445	Moira River	MR5	WHSC		164		70		F	IM	1
Oct-99	446	Moira River	MR5	WHSC		155		45		M	IM	1
Oct-99	447	Moira River	MR5	WHSC		325		430		F	SD	4
Oct-99	448	Moira River	MR5	WHSC		248		190		F	IM	4
Oct-99	449	Moira River	MR5	WHSC		242		190		M	SD	6
Oct-99	450	Moira River	MR5	WHSC		212		120		F	SD	3
Oct-99	451	Moira River	MR5	WHSC		118		20		F	IM	2
Oct-99	452	Moira River	MR5	WHSC		180		75		U	IM
Oct-99	453	Moira River	MR5	WHSC		162		60		U	IM
Oct-99	454	Moira River	MR5	WHSC		139		39		U	IM
Oct-99	455	Moira River	MR5	WHSC		134		40		U	IM
Oct-99	456	Moira River	MR5	WHSC		132		35		U	IM
Oct-99	457	Moira River	F-3	LNDC	MOE99FMR3LNDC457	103	111	11.541	9.626	F	SD	3	0.177	1.157	2468	0.83	0
Oct-99	458	Moira River	F-3	LNDC	MOE99FMR3LNDC458	85	91	6.326	5.233	F	SD	3	0.12	0.651	2054	0.75	0
Oct-99	459	Moira River	F-3	LNDC	MOE99FMR3LNDC459	70	76	3.591	3.013	F	SD	1	0.041	0.306	1260	0.65	0
Oct-99	460	Moira River	F-3	LNDC	MOE99FMR3LNDC460	90	95	7.286	6.114	F	SD	2	0.125	0.642	2096	0.65	0
Oct-99	461	Moira River	F-3	LNDC	MOE99FMR3LNDC461	90	96	6.539	5.452	F	SD	4	0.142	0.643	2088	0.69	0
Oct-99	462	Moira River	F-3	LNDC	MOE99FMR3LNDC462	64	69	3.021	2.715	M	SD	2	0.024	0.043			0
Oct-99	463	Moira River	F-3	LNDC	MOE99FMR3LNDC463	67	72	3.182	2.917	M	SD	1	0.039	0.049			0
Oct-99	464	Moira River	F-3	LNDC	MOE99FMR3LNDC464	68	73	3.155	2.85	M	SD	2	0.019	0.035			50	black mush
Oct-99	465	Moira River	F-3	LNDC	MOE99FMR3LNDC465	76	82	4.448	3.756	F	SD	2	0.075	0.33	1069	0.7	0
Oct-99	466	Moira River	F-3	LNDC	MOE99FMR3LNDC466	75	80	4.4	3.999	M	SD	1	0.05	0.073			0
Oct-99	467	Moira River	F-3	LNDC	MOE99FMR3LNDC467	66	71	2.846	2.623	M	SD	1	0.037	0.045			0
Oct-99	468	Moira River	F-3	LNDC	MOE99FMR3LNDC468	70	75	3.826	3.505	M	SD	2	0.036	0.063			0
Oct-99	469	Moira River	F-3	LNDC	MOE99FMR3LNDC469	72	76	3.995	3.617	M	SD	2	0.05	0.069			0
Oct-99	470	Moira River	F-3	LNDC	MOE99FMR3LNDC470	78	84	4.677	4.256	M	SD	3	0.056	0.73			0
Oct-99	471	Moira River	F-3	LNDC	MOE99FMR3LNDC471	77	82	4.507	3.779	F	SD	2	0.062	0.315	983	0.69	0
Oct-99	472	Moira River	F-3	LNDC	MOE99FMR3LNDC472	70	75	3.433	2.975	F	SD	1	0.037	0.197	862	0.63	0
Oct-99	473	Moira River	F-3	LNDC	MOE99FMR3LNDC473	66	70	3.157	2.812	M	SD	2	0.036	0.049			100	snalls
Oct-99	474	Moira River	F-3	LNDC	MOE99FMR3LNDC474	72	76	3.436	2.912	F	SD	1	0.035	0.215	751	0.63	100	black mush
Oct-99	475	Moira River	F-3	LNDC	MOE99FMR3LNDC475	69	75	3.32	2.988	M	SD	3	0.029	0.06			0	black mush
Oct-99	476	Moira River	F-3	LNDC	MOE99FMR3LNDC476	72	78	3.802	3.391	M	SD	4	0.041	0.067			80	black mush
Oct-99	477	Moira River	F-3	LNDC	MOE99F'LNDC477	77	82	4.286	3.858	M	SD	4	0.052	0.061			100	black mush
Oct-99	478	Moira River	F-3	LNDC	MOE99FMR3LNDC478	63	69	2.633	2.399	M	SD	2	0.026	0.034
Oct-99	479	Moira River	F-3	LNDC	MOE99FMR3LNDC479	71	77	3.662	3.326	M	SD	2	0.043	0.08
Oct-99	480	Moira River	F-3	LNDC	MOE99FMR3LNDC480	73	79	4.404	3.692	F	SD	2	0.055	0.355	1049	0.73	0
Oct-99	481	Moira River	F-3	LNDC	MOE99FMR3LNDC481	75	80	4.497	3.828	F	SD	2	0.081	0.271	1134	0.67	0
Oct-99	482	Moira River	F-3	LNDC	MOE99FMR3LNDC482	64	70	2.733	2.39	F	SD	2	0.049	0.094	321	0.55	0
Oct-99	483	Moira River	F-3	LNDC	MOE99FMR3LNDC483	65	71	3.114	2.702	F	SD	1	0.07	0.191	813	0.7	0
Oct-99	484	Moira River	F-3	LNDC	MOE99FMR3LNDC484	67	72	3.192	2.896	M	SD	1	0.03	0.057			0
Oct-99	485	Moira River	F-3	LNDC	MOE99FMR3LNDC485	85	92	6.124	5.554	M	SD	5	0.082	0.098			0
Oct-99	486	Moira River	F-3	LNDC	MOE99FMR3LNDC486	86	92	6.88	5.556	F	SD	3	0.106	0.761	2468	0.74	0
Oct-99	487	Moira River	F-3	LNDC	MOE99FMR3LNDC487	70	76	3.348	2.936	F	SD	1	0.37	0.194	683	0.69	0
Oct-99	488	Moira River	F-3	LNDC	MOE99FMR3LNDC488	71	77	3.66	3.322	M	SD	2	0.33	0.062			0
Oct-99	489	Moira River	F-3	LNDC	MOE99FMR3LNDC489	70	75	3.688	3.101	F	SD	2	0.064	0.291	1074	0.73	0
Oct-99	490	Moira River	F-3	LNDC	MOE99FMR3LNDC490	83	90	5.779	4.829	F	SD	3	0.077	0.469	1320	0.72	10	black mush
Oct-99	491	Moira River	F-3	LNDC	MOE99FMR3LNDC491	81	88	5.289	4.802	M	SD	3	0.051	0.054			0
Oct-99	492	Moira River	F-3	LNDC	MOE99FMR3LNDC492	83	90	5.877	5.419	M	SD	4	0.041	0.093			0
Oct-99	493	Moira River	F-3	LNDC	MOE99FMR3LNDC493	65	70	3.082	2.857	M	SD	1	0.032	0.052			0
Oct-99	494	Moira River	F-3	LNDC	MOE99FMR3LNDC494	72	78	4.299	3.626	F	SD	2	0.072	0.344	1113	0.78	0
Oct-99	495	Moira River	F-3	LNDC	MOE99FMR3LNDC495	100	108	10.249	8.567	F	SD	3	0.162	0.684	2443	0.7	30	black mush
Oct-99	496	Moira River	F-3	LNDC	MOE99FMR3LNDC496	90	97	7.709	6.385	F	SD	3	0.115	0548	1536	0.69	100	snails
Oct-99	497	Moira River	F-3	LNDC		95		9.489		U	UN	3
Oct-99	498	Moira River	F-3	LNDC		89		7.646		U	UN	2
Oct-99	499	Moira River	F-3	LNDC		48		1.142		U	IM	0
Oct-99	500	Moira River	F-3	LNDC		46		1.081		U	IM	0
Oct-99	501	Moira River	F-3	LNDC		40		0.777		U	IM	0
Oct-99	502	Moira River	F-3	LNDC		41		0.854		U	IM	0
Oct-99	503	Moira River	F-3	LNDC		42		0867		U	IM	0
Oct-99	504	Moira River	F-3	LNDC		44		0.858		U	IM	0
Oct-99	505	Moira River	F-3	LNDC		45		0.881		U	IM	0
Oct-99	506	Moira River	F-3	LNDC		40		0.656		U	IM	0

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