Standard Operating Procedure EAP124, Version 1.4

Watershed Health Monitoring: Standard Operating Procedures for Vertebrate Assemblage Sampling

November 2018 Publication 18-03-228

Purpose of this document

The State Department of Ecology develops Standard Operating Procedures (SOPs) to document agency practices related to sampling, field and laboratory analysis, and other aspects of the agency’s technical operations.

Publication information

This SOP is available on the Department of Ecology’s website at https://fortress.wa.gov/ecy/publications/SummaryPages/1803228.html.

Ecology’s Activity Tracker Code for this SOP is 18-052.

Contact information

For more information contact: Communications Consultant Environmental Assessment Program P.O. Box 47600, Olympia, WA 98504-7600 Phone: 360-407-6764

Washington State Department of Ecology – ecology.wa.gov.

Location of Ecology Offices Phone Headquarters, Lacey 360-407-6000 Northwest Regional Office, Bellevue 425-649-7000 Southwest Regional Office, Lacey 360-407-6300 Central Regional Office, Union Gap 509-575-2490 Eastern Regional Office, Spokane 509-329-3400

Any use of product or firm names in this publication is for descriptive purposes only and does not imply endorsement by the author or the Department of Ecology.

To request ADA accommodation for disabilities, or printed materials in a format for the visually impaired, call Ecology at 360-407-6764 or visit https://ecology.wa.gov/accessibility. People with impaired hearing may call Washington Relay Service at 711. People with speech disability may call TTY at 877-833-6341.

Washington State Department of Ecology

Environmental Assessment Program

Watershed Health Monitoring: Standard Operating Procedures for Vertebrate Assemblage Sampling

Version 1.4

Author -Glenn Merritt

Date –

Reviewer – Shannon Hubler (Oregon DEQ), George Onwumere, and Meghan Rosewood-Thurman

Date –

QA Approval – Tom Gries, Acting Ecology Quality Assurance Officer

Date – September 6, 2018

EAP124

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Please note that the Washington State Department of Ecology’s Standard Operating Procedures (SOPs) are adapted from published methods, or developed by in-house technical and administrative experts. Their primary purpose is for internal Ecology use, although sampling and administrative SOPs may have a wider utility. Our SOPs do not supplant official published methods. Distribution of these SOPs does not constitute an endorsement of a particular procedure or method.

Any reference to specific equipment, manufacturer, or supplies is for descriptive purposes only and does not constitute an endorsement of a particular product or service by the author or by the Department of Ecology.

Although Ecology follows the SOP in most instances, there may be instances in which Ecology uses an alternative methodology, procedure, or process.

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SOP Revision History

Revision Date Version Summary of changes Sections Reviser(s) number 3/10/17 1.1 Updated title, removed draft dates, All Meghan added footers, general formatting, Rosewood- updated glossary terms and references Thurman 3/23/17 1.2 For DCEs with vertebrate data 2.1 Glenn Merritt Last sentence edited 2.2 Reynolds, 1983 3.9 Whiteman, 1994 3.15 Reynolds, 2008 3.16 Refined life stage definition 3.22 Reynolds, 2008 3.27 vertebrate assemblage data 4.1 know the protocol to be used 4.3 wide protocol (if fishing is performe) 6.0 renumbered for raft-based fishing 7.0 added note that method is optional 2017 11.9,11.10 Added link 11.31 Reynolds, 1983 11.34 Reynolds, 2008 11.36 3/27/17 1.3 General formatting All Meghan Rosewood- Thurman 12/11/17 1.4 Clarified wording, added temperature 6.1.4.1 Meghan Added “process salmonids first” and 6.2.2.3 Rosewood- “well aerated” Thurman 9/6/18 1.4 Minor changes (e.g. updated references) Various Gries 11/16/18 1.4 Updated formatting for accessibility, All Ponzetti added cover page

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Environmental Assessment Program

Watershed Health Monitoring: Standard Operating Procedures for Vertebrate Assemblage Sampling

1.0 Purpose and Scope

1.1 This document is the Environmental Assessment Program’s (EAP) Standard Operating Procedure (SOP) for vertebrate assemblage sampling for the Watershed Health Monitoring (WHM) program. It includes methods for both WHM protocols: the Narrow Protocol and the Wide Protocol. Note: This document is derived in large part from methods of the U.S. Environmental Protection Agency’s Environmental Monitoring and Assessment Program, Western Pilot (EMAP-W; see the two Peck et al. manuals (2005a, 2005b) cited in Stoddard et.al., 2005).

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2.0 Applicability

2.1 This SOP should be followed when performing data collection events (DCEs) involving vertebrate community data to be submitted to the WHM Database (see Janisch, 2017). 2.2 This SOP explains how to sample and amphibians to estimate the relative abundance of vertebrate taxa inhabiting a sampling site during a DCE. It is applicable only to projects that also collect a complete set of WHM habitat data, including 11 major transects and 100 thalweg stations. Precede this SOP by defining the site dimensions (Merritt, 2017 or Hartman, 2017a).

3.0 Definitions

3.1 Ambient conductivity: Conductivity (μS/cm) of the water for the ambient water temperature. Electrofishing success depends on ambient conductivity (Ca) rather than specific conductivity (Cs). It can be estimated from specific conductivity with this formula from Reynolds (1996): = /[1.02( )] where Ts = 25°C and Ta= the ambient water temperature in °C. Ambient conductivity𝑇𝑇𝑇𝑇−𝑇𝑇𝑇𝑇 is the most important habitat factor affecting electrofishing efficiency.𝐶𝐶𝐶𝐶 𝐶𝐶𝐶𝐶 3.2 DCE: The Data Collection Event is the sampling event for the given protocol. Data for a DCE are indexed using a code which includes the site ID followed by the year, month, day, and the time (military) for the start time of the sampling event. For example: WAM06600-000222-DCE-YYYY-MMDD-HH:MM. One DCE should be completed within one working day, lasting 4-6 hours, on average. 3.3 Duty cycle: Duty cycle is the percentage of time that the output pulse is “on” during the time period between pulse cycles. On the Smith-Root LR-20 electrofisher, the duty cycle switch is located on the upper left center of the control panel (Figure 1). Increasing duty cycle might increase stress to . Duty cycle is not a feature that can be adjusted on the raft-based electrofisher (Smith-Root GPP, 2007).

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Figure 1. The control panel of the Smith-Root LR-20.

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3.4 EAP: Environmental Assessment Program 3.5 Ecology: Washington State Department of Ecology 3.6 e-forms: Electronic data forms. Term for an application saved into a web browser cache on a device such as a tablet computer. E-forms allow collection and storage of data at remote locations when disconnected from the internet. 3.7 EIM: The Environmental Information Management System (EIM) is the Department of Ecology's main database for environmental monitoring data. EIM contains records on physical, chemical, and biological analyses and measurements. Supplementary information about the data (metadata) is also stored, including information about environmental studies, monitoring locations, and data quality. The “Search by map” feature enables plotting coordinates over orthophotographic imagery. 3.8 Frequency: This describes the pulse rate per second or Hertz (Hz). On the Smith-Root LR-20 electrofisher, the frequency switch is located on upper left of the control panel (Figure 1). Most pulsed DC backpack electrofishing is done at 30-60 Hz. 3.9 Galvanotaxis: This is electrically-induced movement (toward the anode or cathode). When pulsed DC current is supplied to water, fish are electrically induced to swim toward the electrode. This is called galvanotaxis (Reynolds, 1983). 3.10 Habitat units: As assessed for WHM, all habitat units are part of the main channel. They are based on the Hawkins et al. (1993) classification system. Habitat units are “quasi-discrete areas of relatively homogeneous depth and flow that are bounded by sharp physical gradients… Different types of units are usually in close enough proximity to one another that mobile stream organisms can select the type of unit that provides the most suitable habitat” (Hawkins et al. 1993). For WHM, any unit (with two exceptions) must be at least as long as half their wetted width and they must include the thalweg. Plunge pools and dry channels are the exceptions. Plunge pools can be shorter than half their width. Dry channels have no wetted width and only need to occupy a single thalweg station to be counted. Note: When deciding if a feature is long enough to constitute a habitat unit, the length is compared to the wetted width of the full main-channel (exclude side-channels and exclude edge pools). 3.11 HUC: Hydrologic Unit Code assigned by the Geological Survey (USGS, 2016b). Scale depends on number of digits. In Washington State, 4-digit HUCS (also known as subregions) reside within the Pacific Northwest Region (2-digit = HUC 17). Four-digit HUCs that overlap Washington are listed below. • 1701 Kootenai-Pend Oreille-Spokane • 1702 Upper Columbia • 1703 Yakima • 1706 Lower Snake • 1707 Middle Columbia • 1708 Lower Columbia • 1710 Coastal

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• 1711 Puget Sound These 4-digit HUCs are NOT a basis for how WHM allocates monitoring; we use Status and Trends Regions (STRs). The 4-digit HUCs however, serve us as a basis for evaluating aquatic vertebrate species origins (native/alien). 3.12 Major transect: One of 11 equidistant transects across the length of a site. These transects run perpendicular to the thalweg and are labeled as follows: A (furthest downstream), B, C, D, E, F, G, H, I, J, and K (furthest upstream). 3.13 Narcosis: A state of electrically-induced immobility with slack muscles. As fish are induced into galvanotaxis and approach the anode, their reaction changes to narcosis (muscle relaxation and loss of equilibrium). While under narcosis, the fish may continue to swim, upside down, toward the anode. Narcosis can sometimes be achieved near the cathode (Reynolds, 1996). 3.14 Narrow Protocol: The set of Watershed Health Monitoring SOPs that describe data collection at wadeable sites with an average bankfull width of less than 25 m at the index station. 3.15 Paedomorph: This is a mature individual that displays juvenile body characteristics (Whiteman, 1994; e.g. a neotenic Pacific giant salamander). 3.16 Power: This is the energy delivery rate (Reynolds, 2008). Electrofishing can be viewed as a power-based phenomena. Electrofishing effectiveness is based on how much power is transferred to the fish. Power transfer is most efficient when water conductivity closely matches the conductivity of fish flesh (near 100 μS/cm for most species). 3.17 Protocol: A collection of SOPs used to accomplish a DCE. Watershed Health Monitoring uses two protocols: The Narrow Protocol is used for sampling wadeable streams that are less than 25m average bankfull width. The Wide Protocol is used for rivers or streams that are wider than 25m average bankfull width or too deep to wade. 3.18 QAMP: Quality Assurance Monitoring Plan. The QAMP for WHM is Cusimano et al (2006). An updated will be available in 2018. 3.19 Segment: Wetted stream area that is defined between major transects. There are 10 segments in each site. 3.20 Site: A site is defined by the coordinates provided to a sampling crew and the boundaries established by the protocol’s site layout method (Hartman, 2017a (SOP EAP105) for the Wide Protocol; Merritt, 2017 (SOP EAP106) for the Narrow Protocol). Typically, a site is centered on the index station and equal in length to 20 times the average of 5 bankfull width measurements. Sites cannot be longer than 2 km nor shorter than 150 m. Narrow protocol sites range from 150 m to 500 m long. Wide Protocol sites are up to 2 km long and most-frequently longer than 500m . The most downstream end of a site coincides with major transect A; the most upstream end coincides with major transect K. 3.21 SITE ID: Identity code for the proposed sampling site. The Format is WAM06600 - # # # # # #

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• Random sites from the Washington Master Sample have a WAM06600- prefix. • Statewide sentinel sites have a SEN06600- prefix. • Ambient Bioassessment Sites have a BIO06600- prefix 3.22 Species-life stage: The age status for each species captured: juvenile, adult, or unknown. Habitat requirements and characteristics can change for species as their status changes from juvenile to adult. Some species undergo metamorphosis from larvae (e.g. lamprey and frogs). For others, size may be the best indication. In this SOP, most non- game fishes (e.g., sculpin, dace, suckers) are assigned an “unknown” life stage. 3.23 specific conductivity: Electrical conductivity is a measure of water’s ability to conduct electricity, and therefore a measure of ionic activity and content. It is the reciprocal of specific resistivity. Specific conductivity is conductivity adjusted to 25˚ C (reported in μS/cm at 25˚ C). This is what most field conductivity meters report. 3.24 SRR: Salmon Recovery Regions were established by the Governor’s Salmon Recovery Office for management of the recovery of salmonid fish populations that are listed as threatened or endangered by the federal government. A map of SRRs can be found here: https://fortress.wa.gov/dfw/score/score/maps/map_salmon_recovery.jsp. 3.25 Station: Any location within the site where an observation is made or part of a sample is collected. 3.26 STR: Status and Trends Regions (STRs) are based on Salmon Recovery Regions (SRRs) that were described by the Governor’s Salmon Recovery Office (JNRC, 1999). Membership is as follows: • Puget STR Puget Sound, & Hood Canal/Puget Sound SRRs • Coastal STR Coastal SRR • Lower Columbia STR Lower Columbia SRR • Mid Columbia STR Mid Columbia SRR • Upper Columbia STR Upper Columbia SRR • Snake STR Snake SRR • Northeast Wash. STR Northeast Washington SRR • Unlisted STR No SRR identified 3.27 Tetany: A state of electrically-induced immobility with rigid muscles. Tetany is usually achieved near the anode, but sometimes near the cathode. Fish captured before they reach tetany experience a lower risk of injury (Reynolds, 2008). 3.28 Thalweg: Path of a stream that follows the deepest part of the channel (Armantrout, 1998). For WHM, we emphasize Armantrout’s use of the word “path” because the thalweg longitudinal profile excludes (sometimes deeper) side pools that are not part of the dominant flow path. 3.29 Thalweg station: One of one hundred (100) equidistant measurement locations in the thalweg, across the length of a site. For example the thalweg stations at/above each major transect are named as follows: • A0, A1, A2, A3, A4, A5, A6, A7, A8, A9, EAP 124 – Vertebrate Assemblage Sampling – V1.4 – 9/6/18 – Page 9 of 32 Uncontrolled copy when printed

• B0. B1, B2, B3, B4, B5, B6, B7, B8, B9, • C0, C1, C2, C3, C4, C5, C6, C7, C8, C9, • … • J0, J1, J2, J3, J4, J5, J6, J7, J8, J9, and • K0. 3.30 WHM: Watershed Health Monitoring, a status and trends monitoring program within the Environmental Assessment Program at the Washington State Department of Ecology. 3.31 Wide Protocol: The set of WHM SOPs that describes the sample and data collection at non-wadeable sites or sites wider than 25 m bankfull width. It is an abbreviated version of the Narrow Protocol and is typically accomplished by use of rafts. 3.32 WRIA: Water Resources Inventory Area. These are 62 watershed-based management units for the State of Washington. They are mapped here: https://fortress.wa.gov/dfw/score/score/maps/map_wria.jsp.

4.0 Personnel Qualifications/Responsibilities

4.1 This SOP pertains to all Environmental Assessment Program field staff collecting and entering vertebrate assemblage data for WHM. 4.2 All field staff must comply with the requirements of the EAP Safety Manual (Ecology, 2017) 4.3 All field staff must have completed the annual WHM field training and be familiar with the WHM protocol to be used: either the Narrow Protocol or the Wide Portocol. The training includes sampling goals and objectives as defined in the QAMP (Cusimano et al., 2006) 4.4 Field staff must be annually trained to minimize the spread of invasive species. See SOP EAP070 (Parsons et al., 2018).

5.0 Equipment

• polarized sun glasses; caps with visor • electrically insulated gloves • measuring board • photarium • taxonomic keys • buckets or live wells • nets: long-handled dipnet (1/8” mesh) and aquarium net • calipers • loop or magnifying glass

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• polyethylene, wide-mouth jars (250 mL to 500-mL) with ethanol. • digital camera with close-up lens • data recording tablet (fully charged; loaded with WHM e-forms) • backup paper (waterproof) version of forms with number 2 pencil and clip board • Backpack electrofishing gear

o backpack electrofisher unit (e.g. Smith-Root LR-20) o anode with ring (with as large a diameter bore as possible) o abrasive cloth for electrode maintenance o cathode (rat-tail) o electrically insulated waders and wading shoes o battery (fully charged) • Raft-based electrofishing gear

o Electrodes o 2.5 GPP Box o Connecting chords (between GPP Box, foot switch, generator) o foot safety switc o generator, fueled 6.0 Summary of Procedure for backpack electrofishing.

Backpack electrofishing is performed at all Narrow Protocol DCEs. If crews opt to fish at Wide Protocol DCEs, the backpack method is used where the stream is more easily sampled by wading. To preserve sample intergrity, vertebrate sampling is conducted after sampling water chemistry (Hartman, 2017b), sediment chemistry (Hartman, 2017c), invertebrates (Larson, 2018), or periphyton (Larson, 2018). The crew first prepares fishing equipment to best suit stream conditions and minimize harm to fish. Then they walk upstream through the stream site to perform a single-pass electrofishing sampling. The Western Environmental Monitoring and Assessment Program (Stoddard et al., 2005) field methods for sampling the aquatic vertebrate assemblage, including both Peck et al., (2005a & b) manuals, served as a basis for this SOP.

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6.1 Pre-sampling preparations. Training: Prior to the start of the season, get staff trained in the principles and techniques of electrofishing. This will help to minimize harm to fish during the field season. A low-fee, on-line course is often available from the United States Fish and Wildlife Service, National Conservation Training Center (e.g., USFWS, 2016). Carefully read the sampling permits and NOAA (2000) guidance to determine special requirements. Be trained in both roles of electrofishing (operator and netter). Absence of Spawners: Prior to sampling, verify that there are no spawning salmonids present. Use pre-season research on the distribution and timing of runs to help. For example, see SalmonScape (2016) and Status Reviews for Salmon and Steelhead (NOAA, 2016), especially these reports: • NMFS-NWFSC-24 (Appendix C-3 shows coho salmon timing) • NMFS-NWFSC-25 (pages 27-28 show pink salmon timing) • NMFS-NWFSC-27 (pages 16-22 show steelhead timing) • NMFS-NWFSC-32 (pages 25-28 show chum salmon timing) • NMFS-NWFSC-33 (Appendix C, Tables 6,7 show sockeye salmon timing) • NMFS-NWFSC-35 (pages 41-45 show Chinook salmon timing). Perform visual confirmation while on site.

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Electrofisher set up. Ensure components are connected according to manufacturer’s instructions (e.g., Smith-Root, 2012). Be sure to set the on-button timer to zero. Electrofisher log and settings tests. Complete a backpack electrofisher log (e.g. Figure 2) to determine that the instrument settings (Figure 1) will maximize capture efficiency and minimize harm to aquatic vertebrates. The log provides useful guidelines for determining your settings and will help to keep track of settings that work well for each type of stream. Record, electrofisher identity (e.g., serial number), site identity, date and time. Retrieve the temperature and conductivity records from start of the DCE (Wolfe, 2017) by referring to the Electrofisher Page of the e-forms (Figure 3). Measure temperature again immediately prior to fishing, and record the new temperature if warmer. Do not fish if you exceed permit temperature requirements.

Figure 2. Backpack electrofisher log.

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Figure 3. The Electrofisher Page e-form with example data.

Run pre-sampling tests while situated well outside the sampling reach. Evaluate settings to ensure that the audio and light signals are emitting at a standard pace. Check to see that fish are attracted to the anode (wand) with the least possible application of electrical intensity. If captured fish show signs of harm, lower the settings (voltage first; then, if necessary, frequency). NOTE: When ambient conductivity is approximately 100 µS/cm (about the same as most fish flesh), little power is required to effectively fish, For lower conductivity water, higher voltage will be needed, For higher conductivity water, more current will be needed, Details on set-up and testing can be found in the instrument manual (e.g, Smith-Root, 2012). 6.2 Sampling the assemblage by backpack Summary: Wade upstream, sampling all available habitats in proportion to their frequency of occurrence in the site. Spend no more than about 20 minutes in each segment (≤ 3.5 hours total per site). One person operates the electrofisher while another nets the vertebrates. Stop at each major transect (or more frequently) to record the data, and to process and release the . When you stop to process, use a break between habitat units whenever possible. Record data on the Vertebrate Collection Page of the e- forms (Figure 4). Electrofish. Once you have completed the backpack electrofisher log and have determined the optimal electrofisher settings, you may begin sampling. Operate the electrofisher according to manufacturer’s instructions (e.g. Smith-Root, 2012). Enter information on the Electrofisher Page e-form (Figure 4). At the bottom of the site (major transect A), reset the timer (Figure 1) and record the following information, on the Backpack Electrofisher Log (Figure 2): • Gear (press “backpack”) • Water visibility (either “good” or “poor”) • Fishing start time (military) EAP 124 – Vertebrate Assemblage Sampling – V1.4 – 9/6/18 – Page 14 of 32 Uncontrolled copy when printed

• Volts (V) • Frequency (Hz) • Duty cyle (%) 6.2.3.1 Perform a safety check. Before you start, all field staff should acknowledge that they know where the safety switch is located and that they are ready for you to begin. Tell all staff nearby that you are ready to begin electrofishing, then start.

Figure 4. The Vertebrate Collection Page e-form, with example data.

6.2.3.2 Net the vertebrates. If working in open sunlight, netting should be performed while wearing polarized sunglasses and a brimmed cap. Net any vertebrates that move toward the anode, then place the animals into a bucket (live-well) of fresh stream water. The following steps will help to protect specimens from harm: • Net the fish away from the electrodes. • Ensure that your net is empty before fishing. • Minimize animals' exposure to air, sunlight, and handling.

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• Process the live-well contents quickly (at least once per segment). • Do not crowd the live-well. • Keep fresh, well aerated water in the live-well. • Process large fishes first, especially salmonids. Enter collection data. Use the Vertebrate Collection Page e-form (Figure 4) to enter data for each according to species-life stage. Identify each species. Find common names in the Appendix, which includes all taxa encountered by Watershed Health Monitoring staff through 2014. Common names for other taxa can be found by searching the Integrated Taxonomic Information System (ITIS, 2016) or Page et al., (2013). Common names listed are available on the e-form by typing the first 3 characters in the “Common Name” field. NOTES ON IDENTIFICATION: Some useful sources of species identification and range are below. • Corkran and Thoms (2006) • IUCN (2016) • Jones, et al. (2005) • Leonard, et al. (1993) • Lyons, et al. (2006) • Natureserve (2010) • Page and Burr (2011) • Pollard, et al. (1997) • SalmonScape (2016) • Scholz et al. (2009) • Scholz et al. (2010) • USGS (2016a) • Washington Herp Atlas (2009) • Western Native Fish Database (2016) • Wydoski and Whitney (2003) There are cases where we identify taxa to a courser level than species. For example, juvenile lamprey are usually identified to the family level (common name = “LAMPREY (FAMILY)”). Where Pacific giant salamanders and Copes giant salamanders co-occur on the range map, they are usually identified to the genus level (common name = “GIANT SALAMANDER (GENUS)”). Adult frogs (common name = “FROG (ORDER)”, often escape before finer-level identitification can be made. Identify tailed frog larvae to the genus level (common name = “TAILED FROG (GENUS)”). 6.2.5.1 Tally by life-stage (juvenile, adult, unknown) of a each species or taxa. NOTES ON LIFE STAGE: Life stage is mostly needed for permit reporting, to distinguish juvenile and adult salmonids that are listed as threatened or endangered by the National Marine Fisheries Service. Some field data recording “rules-of-thumb” are below: • Chinook salmon < 135 mm are juvenile (Parker and Larkin, 1959).

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• Coho salmon < 290 mm are juvenile (NOAA, 1995). • Cutthroat trout < 150 mm are juvenile (Carlander, 1969). • Cuttroat trout > 180 mm are adult (Carlander, 1969). • Rainbow trout < 150 mm are juveniles (Scott and Crossman, 1973). • Rainbow trout > 250 mm are adult (Scott and Crossman, 1973). • Bull trout < 150 mm are juvenile (Rieman and McIntyre, 1993). • Bull trout > 300 mm are recorded as adult (permit language). • Brook trout are recorded as unknown life stage. • Lamprey with hidden eyes & toothless are juvenile (Scholz et al., 2010). • Frogs/Toads as tadpoles (legs not fully formed) are juvenile. • Salamanders as larvae/paedomorphs are recorded as juvenile. • Other non-salmon fishes are reported as unknown life stage. 6.2.5.1.1 Record any new segment of encounter (A,B, C, ..J), and 6.2.5.1.2 Record length (mm) of the animal if it is the smallest or largest yet for the species-life stage in the DCE. NOTES ON LENGTH: We measure “natural” total length in most cases. This is the length from the most anterior part of the animal, to the most posterior extent of its tail, with the tail not pinched but resting in a “natural position” (Anderson and Gutreuter, 1983). However, adult frogs and toads are measured from snout-to-vent. 6.2.5.1.3 Tally any unintentional mortalities that resulted from fishing activities. NOTE: Whenever you detect any harm to fish, re-evaluate the fishing methods. You might reduce power, decrease handling time, or cease fishing. Photograph. Document each species life-stage that is encountered, focusing on key features for (see Lyons et al., 2006; Stauffer et al., 2001) Collect voucher specimens. These are retained for later identification in a laboratory or by a professional taxonomist. 6.2.7.1 Target difficult-to-identify species (e.g., members of , , Cyprinidae, or non-native species). Do not mix species in any jar. Also, you should only need to use one jar per species. Do not save any of the examples below. Plenty of good photographs should suffice. • No large specimens that won’t fit into a 500 mL wide-mouth jar • No salmonids (except in cases of mortality as required by permits). • No amphibians • No lamprey 6.2.7.2 Add ethanol according to the method of Bean (1882). Fill each jar with ethanol by diluting a 95% stock solution (2:1) in water, including the fish. NOTE: After a day or two, rinse specimens and replace ethanol with a stronger solution (3:1 of ethanol to water).

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6.2.7.3 Label each jar. Complete 2 Voucher Jar Tags (Figure 5) using a number 2 pencil and waterproof paper. Tape one to the exterior, and insert one to the interior. 6.2.7.4 Seal each jar lid securely using electrical tape. Write a consecutive jar identity number (for your crew, per year) on the jar lid. 6.2.7.5 Photograph the jar with label and jar id.

DCE WAM06600-000000-DCE-2019-0730-11:00 STREAM LOST RIVER TRIBUTARY COMMON NM LONGNOSE DACE (2) (COUNT) ITIS SERIAL NO. SN 163384 TL (mm) 68 mm, 72 mm METHOD BACKPACK ELECTROFISHER COLLECTOR JANE DOE (JAR # 22) (JAR ID) Figure 5. Voucher Jar Tag with example data.

6.2.7.5.1 Normally, this is the same as site length, however it might be shorter than site length if you had to avoid areas for safety reasons or for permit reasons. 6.2.7.5.2 For sites with dry patches, do NOT subtract those distances from site length. Wetted area information will be available from the habitat survey (other SOPs). 6.2.7.6 Verify that the settings on the e-form for Volts, Frequency and Duty Cycle are accurate by examining the control panel display (Figure 1). Release all other animals alive. Find quiet water at a location well below the next electrofishing activity. Do this frequently to avoid holding animals any longer than necessary. Finalize the Electrofisher Page. When you have finsished electrofishing the entire site (or as much as possible), complete the Electrofisher Page e-form (Figure 3). 6.2.9.1 Record final clock time (military). 6.2.9.2 Record on-button time (seconds) from the display of the electrofisher control panel (Figure 1). Once recorded, zero out the timer prior to the next DCE. 6.2.9.3 Record final distance sampled (m) for the site.

7.0 Summary of Procedure for raft-based electrofishing.

Sampling the vertebrate assemblage is otional for sites sampled using the Wide Protocol. As of 2017, we normally do not fish these sites. In special circumstances when the project opts to fish, then raft-based electrofishing is performed where wading is impractical. The electrofishing raft (biology crew) follows the habitat raft so that they

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can see where transects are located (the habitat boat will be navigating to each transect with the GPS). The crew first prepares their fishing equipment to best suit the stream conditions and to minimize stress to fish. They then float down through the stream site (Transect K to Transect A) to perform a single-pass electrofishing sampling. The crew processes animals and enters data at each major transect. NOTE: To preserve sample integrity, electrofish within each segment only after completing any sampling for water chemistry (Hartman, 2017b), sediment chemistry (Hartman, 2017c), invertebrates (Larson, 2018) or periphyton (Larson, 2018). 7.1 Pre-sampling preparations. Training: Refer to 6.1.1. Practice sessions should be performed prior to sampling, at a location external to the range of threatened or endangered species. Additional training is required for safe operation of rafts; see the latest Environmental Assessment Program Safety Manual (Ecology, 2015). Absence of spawners: Refer to 6.1.2 Electrofisher set up. Ensure components are connected according to manufacturer’s instructions (Smith-Root, 2007), as needed for the raft (Figure 6).

Figure 6. Raft-based electrofisher set-up (from Smith-Root, 2007).

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Electrofisher log and settings tests. 7.1.4.1 Complete a raft electrofisher log (Figure 7) to determine that the electrofishing equipment is working properly. Adjust the 2.5 GPP box settings on the control panel (Figure 8) to maximize capture efficiency and minimize harm to aquatic vertebrates. The log provides useful guidelines for determining your settings and will help to keep track of settings that work well for each type of river. Record, electrofisher identity (e.g., serial number), site identity, date and time. Retrieve the temperature and conductivity records from start of the DCE (Wolfe, 2017) by referring to the (raft) Electrofisher Page of the e-forms (Figure 9).

Figure 7. Raft electrofisher log.

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Figure 8. The Smith-Root 2.5 GPP control panel

Figure 9. The electrofisher e-form page for raft-based electrofishing, with example data.

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7.1.4.1.1 Establish initial settings on the the raft-based electrofisher control panel (Figure 8). Set: • Emergency OFF switch in the “up” position, • Voltage Range to LOW (50-500), • Percent of Power at 60%, • Mode on DC • Pulses per second on 30 (pps=Hz) 7.1.4.1.2 Test your initial setting and examine the output ammeter (Figure 8, #2). It should read between 2-4 amps. If this is less than 2 amps, start turning up the dials. Perform your test while situated well upstream of the sample site. 7.1.4.1.3 First increase pulse rate to 60 pps. If that does not work, then incrementally increase power settings to 80%, then 100%. until you display 2-4 amps, and attract fish with minimal signs of stress to them. 7.1.4.1.4 If that does not work, then set Power back to 40% and increase voltage range to High (50-1000). Work through the same progression with the range on high until you display 2-4 amps, and attract fish with minimal signs of stress to them. NOTE: Check that fish are attracted to the anodes. Record in the log note book, the fish responses to each of the different control panel settings and ammeter results. If fish demonstrate signs of stress, lower the settings. NOTE: When ambient conductivity is approximately 100 uS/cm (similar to fish flesh for many species), little power is required to effectively fish. For lower conductivity water, higher voltage will be needed. For higher conductivity water, settings providing more current will be needed (e.g., higher voltage or frequency). Refer to the 2.5 GPP manual (e.g. Smith-Root, 2007) 7.2 Sampling the assemblage by raft-based electrofishing. Float downstream through the site, sampling all available littoral (margin) habitats in proportion to their frequency of occurrence in the site (but avoiding safety hazards). One person navigates the boat and operates the electrofisher. Another person nets the vertebrates and empties the net into an uncrowded live-well with fresh, cold water. Stop at every major transect to process and release the animals. Record data on the Vertebrate Collection Page e-form. (Figure 4). Electrofish. Once you have completed the raft electrofisher log and have determined the optimal electrofisher settings, you may begin sampling. Operate the electrofisher according to manufacturer’s instructions (e.g. Smith-Root, 2007). 7.2.2.1 Start the Electrofisher Page e-form for raft (Figure 9). While beached at the top of the site (major transect K), reset the timer (Figure 8, #7) and record the following information: • Gear (press “raft”) • Water visibility (either “good” or “poor”) • Fishing start time (military) • Volts (max of range x % of range) • Frequency in Hz (pulses per second) EAP 124 – Vertebrate Assemblage Sampling – V1.4 – 9/6/18 – Page 22 of 32 Uncontrolled copy when printed

• Duty Cycle (not applicable for raft; enter a “0” dummy value) 7.2.2.2 Discuss communication plans for use of hand signals (the generator is loud and ear protection is recommended). Verify there are no persons, pets, or livestock in the water. The electrofisher/boat operator should announce their intent to begin, and then start. 7.2.2.3 Net the vertebrates. If working in open sunlight, netting should be performed while wearing polarized glasses and brimmed headwear. Net any vertebrates that move toward the anode arrays. Empty the net contents into a live-well of fresh river water. The following steps will help to protect animals from harm: • Net the fish before they contact the anodes • Ensure that your net is empty before fishing • Minimize the animals’ exposure to air, sunlight, and handling • Process the live-well at least at every major transect • Do not crowd the live-well. • Keep fresh water in the live-well. • If you see an adult salmon or a bull trout in the water, leave it alone, turn off the power, and float away. Enter collection data. Use the Vertebrate Collection Page e-form (Figure 4) to enter data for each animal according to species life-stage. 7.2.3.1 Identify and document each species life-stage as in 6.2.3.1, and 6.2.3.2. Photograph each species life-stage that is encountered, focusing on key features for taxonomy (see Lyons et al. (2006), Stauffer et al., (2001)). Collect voucher specimens as in 6.2.5.

8.0 Release Unretained Animals

8.1 Release unretained animals alive in quiet water, away from the next fishing activity. Do this frequently (at least once every segment) to minimize stress. 8.2 Finalize the Electrofisher Page e-form as in 6.2.7.

9.0 Records Management

9.1 Refer to the SOP EAP125, Managing Electronic Data Form Functionality for Watershed Health Studies (Janisch, 2017). 9.2 Ensure that labels are complete for all voucher specimen jars and add a jar number to the lid (unique to your sample crew). Photograph the jar including a clear image of the labels. Maintain a spreadsheet manifest of voucher jars that includes information about the site and the specimens, including: • Jar number • DCE • Site description (as in EIM or as to be submitted there) • HUC4

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• STR • WRIA • County • Latitude & Longitude (decimal degrees) • Town-Range-Section (as in EIM) • ITIS serial number • Common name (as in ITIS) • Scientific name (as in ITIS) • List of Total Lengths (mm) for all specimens in jar. • Sampling method (backpack electrofishing, or boat electrofishing) • Collector (first and last name of person identified during DCE) 9.3 Download voucher photographs and jar photographs to a local hard drive following every DCE. These should be backed up to a network drive.

10.0 Quality Control and Quality Assurance

10.1 PROJECT QA/QC is discussed in the Quality Assurance Monitoring Plan (Cusimano et al., 2006), will be updated in 2018. 10.2 SAMPLING PRECISION: Repeat the sampling for 10% of all sites per year per Status and Trends Region. Timing of replicates should be several weeks or more following initial samples (as far apart in time as possible but within the same index period). 10.3 SAMPLING ACCURACY: Photograph all species and review features before identity data are certified. Review voucher specimens for select fishes. Use professional taxonomists whenever possible. Maintain voucher samples in ethanol so that DNA analysis later can be performed if possible. 10.4 REPRESENTATIVENESS: 10.5 Sample the site equally across fishable surface area. Sample habitats in proportion to their occurrence. If possible, electrofish on the same day that habitat data are collected.

11.0 Safety

11.1 All field staff must comply with the requirements of the EAP Safety Manual (Ecology, 2017).

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12.0 References

Anderson, R.O. and S.J. Gutreuter. 1983. Length, weight, and associated structural indices. Pages 284-300 in L.Nielsen and D. Johnson (eds.) Fisheries Techniques, American Fisheries Society, Bethesda, Maryland. Armantrout, N.B. compiler. 1998. Glossary of aquatic habitat inventory terminology. American Fisheries Society, Bethesda, Maryland. Bean, Tarleton, H. 1882. Proceedings of the United States National Museum for 1881 (Washington: Government Printing Office) pages 135-238. [An exerpt may be found here: http://tinyurl.com/BeanETOH.] Carlander, K.D., 1969. Handbook of freshwater fishery biology, volume 1. The Iowa State University Press, Ames. Iowa. 752 p. Corkran, C. C. and C. Thoms. 2006. Amphibians of Oregon, Washington and (Revised and Updated edition). Lone Pine, Redmond, Washington. 176 pp. Cusimano, R., G. Merritt, R. Plotnikoff, C. Wiseman, C. Smith, and WDFW. 2006. Status and Trends Monitoring for Watershed Health and Salmon Recovery: Quality Assurance Monitoring Plan. https://fortress.wa.gov/ecy/publications/SummaryPages/0603203.html. Ecology, 2017. Environmental Assessment Program Safety Manual. Washington State Department of Ecology. Olympia, WA. Hartman, C. 2017a. Watershed Health Monitoring: Standard Operating Procedures for GIS-Based Verification, Layout, and Data Collection (Wide Protocol). SOP EAP105. Washington State Department of Ecology, Environmental Assessment Program, Olympia. http://ecology.wa.gov/programs/eap/quality.html. Hartman. C. 2017b. Watershed Health Monitoring: Standard Operating Procedures for Collecting Water Samples. SOP EAP095. Washington State Department of Ecology, Environmental Assessment Program, Olympia. http://ecology.wa.gov/programs/eap/quality.html. Hartman. C. 2017c. Watershed Health Monitoring: Standard Operating Procedures to Sample Sediment for Chemistry. SOP EAP110. Washington State Department of Ecology, Environmental Assessment Program, Olympia. http://ecology.wa.gov/programs/eap/quality.html. Hawkins, C.P., J.L. Kershner, P.A. Bisson, M.D. Bryant, L.M. Decker, S.V. Gregory, D.A. McCullough, C.K. Overton, G.H. Reeves, R.J. Steedman, and M.K. Young. 1993. Hierarchical approach to classifying stream habitat features. Fisheries 18:3-12. ITIS. 2016. The Integrated Taxonomic Information System, [Accessed April 19, 2016]. http://www.itis.gov IUCN. 2016. The IUCN Red List of Threatened Species. International Union for Conservation of Nature, Internet pages [accesed April 26, 2016]. http://maps.iucnredlist.org

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Janisch, J. 2017. Standard Operating Procedures for Managing Electronic Data Form Functionality for Watershed Health Studies using a Mobile Data-Collection Device. SOP EAP125. Washington State Department of Ecology, Olympia, WA http://ecology.wa.gov/programs/eap/quality.html JNRC. 1999. Statewide Strategy to Recover Salmon – Extinction is Not an Option, Chapter III: A Road Map to Recovery. Governor’s Salmon Recovery Office, Olympia, WA. http://digitalarchives.wa.gov/governorlocke/gsro/strategy/summary/roadmap.htm Jones, L.L.C., W.P. Leonard and D.H. Olson (Coordinating Editors). 2005. Amphibians of the Pacific Northwest. Seattle Audubon Society, Seattle, Washington. Larson, C. 2018. Standard Operating Procedures and Minimum Requirements for the Collection of Freshwater Benthic Macroinvertebrates in Streams and Rivers, Version 2.1. SOP EAP073. Washington State Department of Ecology, Olympia, WA. http://ecology.wa.gov/programs/eap/quality.html Larson, C. 2018. In Press. Watershed Health Monitoring, Standard Operating Procedures (SOP) for Sampling the Periphyton Assemblage, Version 1.0. SOP EAP111. Washington State Department of Ecology, Olympia, WA. http://ecology.wa.gov/programs/eap/quality.html Leonard, W.P., H.A. Brown, L.L.C. Jones, K.R. McAllister and R.M. Storm. 1993. Amphibians of Washington and Oregon. Seattle Audubon Society, The Trailside Series, Seattle, Washington. 168 pp. Lyons, J., P. Hanson, and E.White. 2006. A photo-based computer system for identifying Wisconsin fishes. Fisheries 31.6 (2006): 269-275. http://www.seagrant.wisc.edu/home/Default.aspx?tabid=604. Merritt, G. 2017. Watershed Health Monitoring: Standard Operating Procedures for Verification and Layout of Sites (Narrow Protocol) SOP EAP106. Washington State Department of Ecology, Environmental Assessment Program, Olympia. http://ecology.wa.gov/programs/eap/quality.html NatureServe. 2010. Digital Distribution Maps of the Freshwater Fishes in the Conterminous United States. Version 3.0. Arlington, VA. U.S.A. http://explorer.natureserve.org NOAA. 1995. Status Review of Coho Salmon from Washington, Oregon, and California. NOAA Technical Memorandum NMFS-NWFSC-24. Appendix C-5: Coho Salmon Spawner Sizes. National Oceanic and Atmospheric Administration, National Marine Fisheries Service. https://www.nwfsc.noaa.gov/publications/scipubs/techmemos/tm24/appc5.htm NOAA. 2000. Guidelines for Electrofishing Waters Containing Salmonids Listed Under the Endangered Species Act. National Marine Fisheries Service, Portland, OR. http://www.westcoast.fisheries.noaa.gov/publications/reference_documents/esa_refs/sec tion4d/electro2000.pdf

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NOAA, 2016. Salmon and Steelhead ESA Status Reviews (Internet Page), National Oceanic and Atmospheric Administration, National Marine Fisheries Service. [Accessed April 25, 2016] https://www.nwfsc.noaa.gov/trt/pubs_statusreview.cfm. Page, L.M. and B.M. Burr. 2011. Peterson Field Guide to Freshwater Fishes of North America North of Mexico. Houghton Mifflin Harcourt, 2011. 688 pp. Page, L.M., H. Espinosa-Pérez, L.T. Findley, C.R. Gilbert, R.N. Lea, N.E. Mandrak, R.L. Mayden, and J.S. Nelson. 2013. Common and scientific name of fishes from the United States, Canada, and Mexico. 7th edition. Bethesda, Maryland: American Fisheries Society, Special Publication 34. Parker, R.R. and P.A. Larkin. 1959. A concept of growth in fishes. J. Fish. Res. Bd. Canada 16(5): 721-745. Parsons, J., D.Hallock, K.Seiders, B.Ward, C.Coffin, E.Newell, C.Deligeannis, and K. Welch. 2018. Standard Operating Procedures to Minimize the Spread of Invasive Species, SOP EAP070. Version 2.1 http://ecology.wa.gov/programs/eap/quality.html Peck, D. V., Averill, D. K., Herlihy, A. T., Hughes, R. M., Kaufmann, P. R., Klemm, D. J., Lazorchak, J. M., McCormick, F. H., Peterson, S. A., Cappaert, M. R., Magee, T. & Monaco, P. A. 2005a. Environmental Monitoring and Assessment Program - Surface Waters Western Pilot Study: Field Operations Manual for Non-Wadeable Rivers and Streams. EPA Report EPA 600/R-05/xxx, U.S. Environmental Protection Agency, Washington, DC. Peck, D. V., Herlihy, A. T., Hill, B. H., Hughes, R. M., Kaufmann, P. R., Klemm, D. J., Lazorchak, J. M., McCormick, F. H., Peterson, S. A., Ringold, P. L., Magee, T. & Cappaert, M. R. 2005b. Environmental Monitoring and Assessment Program - Surface Waters Western Pilot Study: Field Operations Manual for Wadeable Streams. EPA Report EPA 600/R-05/xxx, U.S. Environmental Protection Agency,Office of Research and Development, Washington, DC. Pollard, W.R. and G. F. Hartman, C. Groot, and P. Edgell. 1997. Field Identification of Coastal Juvenile Salmonids. Harbour Publishing, Madeira Park, British Columbia, Canada, 32 p. Rieman, B. E., and J. D. McIntyre. 1993. Demographic and habitat requirements for conservation of bull trout. USDA Forest Service, Intermountain Research Station, Gen. Tech. Rep. INT-302. 38 pp. http://www.fs.fed.us/rm/pubs_int/int_gtr302.pdf Reynolds, J.B. 1983. Electrofishing. Pages 147-163 in L.A. Neilsen and D.L. Johnson, editors. Fisheries techniques. American Fisheries Society, Bethesda, Maryland. Reynolds, J. B. 1996. Electrofishing. Pages 221–254 in B. R. Murphy and D. W. Willis, editors. Fisheries techniques, 2nd edition. American Fisheries Society, Bethesda, Maryland. Reynolds, J.B. 2008. Backpack Electrofoshing and Fish Handling Techniques: Effective Methods for Maximizing Fish Capture and Survival. Northwest Environmental Training Center Course ID: BIO-407, September 16-18, 2008, Seattle, WA.

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SalmonScape. 2016. Interactive map. Washington Department of Fish and Wildlife. [Accessed April 22, 2016] http://wdfw.wa.gov/mapping/salmonscape/ Scholz, A.T.; H.J. McLellan, J.McMillan, L. Conboy, M.Kirkendall, and A.Davis. 2009. Field Guide to the Fishes of Eastern Washington. Eastern Washington University, Biology Faculty Publications Paper 11. http://dc.ewu.edu/biol_fac/11 Scholz, A.T., H.J. McLellan, and Fisheries Research Center, Eastern Washington University. 2010. Fishes of the Columbia and Snake River Basins in Eastern Washington. Eastern Washington University, Biology Faculty Publications Paper 16. http://dc.ewu.edu/biol_fac/16 Scott, W.B. and E.J. Crossman. 1973. Freshwater fishes of Canada. Bull. Fish. Res. Board Can. 184:1-966. Smith-Root. 2007. User’s Manual: GPP 2.5, 5.0, 7.5, & 9.0 Portable Electrofishers. Smith-Root, Inc, Vancouver, WA. http://www.smith-root.com/support/downloads/manuals Smith-Root. 2012. User’s Manual: LR-20B Backpack Electrofisher. Smith-Root, Inc, Vancouver, WA. http://www.smith-root.com/support/downloads/lr-20-series- electrofisher-manual/ Stauffer, J.R., J. Karish, and T.D. Stecko. 2001. Guidelines for Using Digital Photos as Fish Vouchers for Pennsylvania Fishes. The Pennsylvania State University and National Park Service. 16 pp. http://partnerweb/sites/EAP/stream/trainingMaterials/VoucherPhotos.pdf Stoddard, J. L., D. V. Peck, S. G. Paulsen, J. Van Sickle, C. P. Hawkins, A. T. Herlihy, R. M. Hughes, P. R. Kaufmann, D. P. Larsen, G. Lomnicky, A. R. Olsen, S. A. Peterson, P. L. Ringold, and T. R. Whittier. 2005. An Ecological Assessment of Western Streams and Rivers. EPA 620/R-05/005, U.S. Environmental Protection Agency, Washington, DC. https://archive.epa.gov/emap/archive- emap/web/html/wstriv.html USFWS. 2016. Principles and Techniques of Electrofishing – Online (Course Number CSP2C01). United States Fish and Wildlife Service, National Conservation Training Center. http://training.fws.gov/topic/online-training/ USGS. 2016a. Nonindigenous aquatic species. United States Geological Survey, NAS Program, Gainesville, FL [Accessed April 21, 2016] http://nas.er.usgs.gov/ USGS. 2016b. Science in Your Watershed. United States Geological Survey, Reston, Virginia [Accessed 21 April, 2016]. http://water.usgs.gov/wsc/reg/17.html. Washington Herp Atlas. 2009. Washington Natural Heritage Program, Washington Dept. of Fish & Wildlife, and U.S.D.I. Bureau of Land Management [accessed 21 April 2016] http://wdfw.wa.gov/conservation/herp_atlas/

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Western Native Fish Database. 2016. Western Division of the American Fisheries Society [accessed 21 April, 2016] http://wdafs.org/awards/western-native-fishes-database/ with links to https://databasin.org/galleries/cceaaf48a4084e93ad0bb40dc4d755f7 Whiteman, H. 1994. Evolution of Facultative Paedomorphosis in Salamanders. The Quarterly Review of Biology, 69(2), 205-221. Wolfe, J. 2017. Watershed Health Monitoring: Standard Operating Procedures for Collecting In Situ Water Quality. SOP EAP108. Washington State Department of Ecology, Olympia, WA.. http://ecology.wa.gov/programs/eap/quality.html Wydoski, R.S., and R.R. Whitney. 2003. Inland Fishes of Washington. 2nd ed. American Fisheries Society and University of Washington Press, Seattle, Washington. 322 pp.

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13.0 APPENDIX A

Table A1. Common names, serial numbers, and origins of previously seen amphibian taxa, by family. Serial Origin by HUC 17__ __ Common name Family No 01 02 03 06 07 08 10 11 FROG (ORDER) 173423 U U U U U U U U WESTERN TOAD Bufonidae 773513 N N N N N N N N CHORUS FROG (GENUS) Hylidae 173523 U U U U U U U U PACIFIC CHORUS FROG Hylidae 207313 N N N N N N N N TAILED FROG (GENUS) Leiopelmatidae 173545 U N N N N N N N AMERICAN BULLFROG Ranidae 775084 A A A A A A A A CASCADES FROG Ranidae 173450 U N N U N N N N COLUMBIA SPOTTED FROG Ranidae 550546 N N U N U U U U NORTH AMERICAN TRUE FROG (GENUS) Ranidae 773285 U U U U U U U U NORTHERN LEOPARD FROG* Ranidae 775108 N N N N N A A A NORTHERN RED-LEGGED FROG Ranidae 173446 U U U U N N N N TRUE FROG (GENUS) Ranidae 173434 U U U U U U U U SALAMANDER (ORDER) 173584 U U U U U U U U GIANT SALAMANDER (GENUS) Ambystomatidae 173740 U U U U U U U U LONG-TOED SALAMANDER Ambystomatidae 173601 N N N N N N N N NORTHWESTERN SALAMANDER Ambystomatidae 173597 U U N U N N N N PACIFIC GIANT SALAMANDER Ambystomatidae 550242 U N N U N N N N CASCADE TORRENT SALAMANDER Rhyacotritonidae 550250 U U U U N N N N COLUMBIA TORRENT SALAMANDER Rhyacotritonidae 550251 U U U U U N N U NEWT AND SALAMANDER (FAMILY) Salamandridae 173613 U U U U U U U U ROUGH-SKINNED NEWT Salamandridae 173620 U U N U N N N N Serial number is from ITIS (2016). Origin is relative to data in USGS (2016a), IUCN (2016). *Origin for northern leopard frog is based on Washington Herp Atlas (2009).

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Table A2. Common names, serial numbers, and origins of previously seen fish taxa, by family. Origin by HUC 17 __ __ Common name Family Serial No 01 02 03 06 07 08 10 11 BRIDGELIP SUCKER Catostomidae 163897 N N N N N N A A Catostomidae 163896 N N N N N N N N LONGNOSE SUCKER Catostomidae 163894 N N A N A A A N MOUNTAIN SUCKER Catostomidae 163909 A N N N N N A A SUCKER (FAMILY) Catostomidae 163892 U U U U U U U U BLACK CRAPPIE Centrarchidae 168167 A A A A A A A A BLUEGILL Centrarchidae 168141 A A A A A A A A GREEN SUNFISH Centrarchidae 168132 A A A A A A A A LARGEMOUTH BASS Centrarchidae 168160 A A A A A A A A PUMPKINSEED Centrarchidae 168144 A A A A A A A A ROCK BASS Centrarchidae 168097 A A A A A A A A SMALLMOUTH BASS Centrarchidae 550562 A A A A A A A A COASTRANGE SCULPIN Cottidae 167230 A A A A N N N N COLUMBIA SCULPIN Cottidae 643936 U N U U U N U U FRESHWATER SCULPIN (GENUS) Cottidae 167229 U U U U U U U U MALHEUR SCULPIN Cottidae 643931 A A A A A A A A MARGINED SCULPIN Cottidae 167247 A A A N N A A A MOTTLED SCULPIN Cottidae 167237 N N N N N N A A PAIUTE SCULPIN Cottidae 167238 A N N N N A A A PRICKLY SCULPIN Cottidae 167233 A N A N N N N N RETICULATE SCULPIN Cottidae 167248 A A A A N N N N RIFFLE SCULPIN Cottidae 167234 A A A A N N N N SHORTHEAD SCULPIN Cottidae 167240 N N N A N N N N SLIMY SCULPIN Cottidae 167232 N N A A A A A A TORRENT SCULPIN Cottidae 167252 A A A A N N N N CHISELMOUTH Cyprinidae 163531 N N N N N N A A COMMON CARP Cyprinidae 163344 A A A A A A A A DACE (GENUS) Cyprinidae 163381 U U U U U U U U FATHEAD MINNOW Cyprinidae 163517 A A A A A A A A LEOPARD DACE Cyprinidae 163386 A N N A A N A A LONGNOSE DACE Cyprinidae 163384 N N N N N N A A NORTHERN PIKEMINNOW Cyprinidae 163523 N N N N N N N N PEAMOUTH Cyprinidae 163521 N N N N N N N N REDSIDE SHINER Cyprinidae 163528 N N N N N N N N SPECKLED DACE Cyprinidae 163387 N N N N N N N N TENCH Cyprinidae 163348 A A A A A A A A NORTHERN PIKE Esocidae 162139 A A A A A A A A BANDED KILLIFISH Fundulidae 165646 A A A A A A A A

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Origin by HUC 17 __ __ Common name Family Serial No 01 02 03 06 07 08 10 11 BROOK STICKLEBACK Gasterosteidae 166399 A A A A A A A A THREESPINE STICKLEBACK Gasterosteidae 166365 N N N N N N N N BLACK BULLHEAD Ictaluridae 164039 A A A A A A A A BROWN BULLHEAD Ictaluridae 164043 A A A A A A A A WALLEYE Percidae 650173 A A A A A A A A YELLOW PERCH Percidae 168469 A A A A A A A A SAND ROLLER Percopsidae 164410 A N N N N N A A LAMPREY (FAMILY) Petromyzontidae 159697 U U U U U U U U PACIFIC LAMPREY Petromyzontidae 159707 N N N N N N N N WESTERN BROOK LAMPREY Petromyzontidae 159707 A A N A N N N N WESTERN MOSQUITOFISH Poeciliidae 165878 A A A A A A A A BROOK TROUT Salmonidae 162003 A A A A A A A A BROWN TROUT Salmonidae 161997 A A A A A A A A BULL TROUT Salmonidae 162004 N N N N N N N N CHINOOK SALMON Salmonidae 161980 A N N N N N N N COHO SALMON Salmonidae 161977 A N N N N N N N CUTBOW Salmonidae none U U U U U U U U CUTTHROAT TROUT Salmonidae 161983 N N N N N N N N MOUNTAIN WHITEFISH Salmonidae 162009 N N N N N N N N PACIFIC SALMON (GENUS) Salmonidae 161974 U U U U U U U U RAINBOW TROUT Salmonidae 161989 N N N N N N N N SOCKEYE SALMON Salmonidae 161979 N N N N N N N N TROUT/SALMON (FAMILY) Salmonidae 161931 U U U U U U U U Serial number is from ITIS (2016). Origin is relative to data in USGS (2016a), Natureserve (2010).

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