Collect and Preserve Specimens

Collect and preserve insect specimens following museum-grade standards including legal compliance, collection methods, humane dispatch, dry pinning, wet preservation, labeling, storage, and curation. Covers permit requirements, protected species regulations, sweep nets, beating trays, pitfall traps, light traps, Malaise traps, aspirators, ethyl acetate killing jars, freezing, pin placement by order, wing spreading, ethanol preservation for soft-bodied specimens, specimen labeling with locality and date, storage with pest management, and database entry. Use when building a reference collection for taxonomic study, preserving voucher specimens for ecological research, preparing specimens for identification by specialists, or curating an existing collection.

Procedure

Step 1: Verify Legal Requirements

Before any collection activity, confirm that you have the legal right to collect at the site and that your target taxa are not protected.

FUNDAMENTAL RULE:
Never collect without proper authorization. Never collect from
protected areas without explicit permits. Never collect protected
species. The scientific value of a specimen is zero if it was
collected illegally — it cannot be published, deposited in a
museum, or used in formal research.

Legal Checklist:
+--------------------+------------------------------------------+
| Requirement        | Verify                                   |
+--------------------+------------------------------------------+
| Land access        | Written permission from landowner, or    |
|                    | site is publicly accessible for          |
|                    | collecting (many parks prohibit it)      |
+--------------------+------------------------------------------+
| Collection permit  | Required for most public lands, nature   |
|                    | reserves, national parks. Apply through  |
|                    | the managing agency. Specify taxa,       |
|                    | methods, dates, and quantities.          |
+--------------------+------------------------------------------+
| Protected species  | Check national and regional red lists,   |
|                    | CITES appendices, and local endangered   |
|                    | species legislation. Some butterflies,   |
|                    | beetles, and dragonflies are protected.  |
+--------------------+------------------------------------------+
| Export/import      | Moving specimens across international    |
|                    | borders requires phytosanitary           |
|                    | certificates and may require CITES       |
|                    | permits depending on the taxon.          |
+--------------------+------------------------------------------+
| Institutional      | If collecting for an institution, follow |
| protocols          | their collection policy and ethics       |
|                    | review requirements.                     |
+--------------------+------------------------------------------+

Minimizing Collection Impact:
- Collect only the minimum number of specimens needed
- Avoid collecting from small or isolated populations
- Do not collect gravid (egg-bearing) females if population is small
- Record the abundance at the site — if the species appears rare, photograph instead
- Prefer common and abundant species for teaching collections

Expected: All required permits are obtained, protected species lists have been checked, and the collector has a clear understanding of what may and may not be collected at the site.

On failure: If permits cannot be obtained, do not collect. Photograph specimens in situ and use citizen science platforms for identification. If a collected specimen turns out to be a protected species, consult the relevant wildlife authority immediately. Do not discard the specimen — accidental collection should be reported, not concealed.

Step 2: Select Collection Method

Choose the method that matches your target taxa, habitat, and research objectives. Different methods sample different portions of the insect community.

Collection Methods:
+--------------------+------------------------------------------+
| Method             | Best For                                 |
+--------------------+------------------------------------------+
| Sweep net          | Flying and vegetation-dwelling insects    |
|                    | in grasslands, meadows, and low shrubs.  |
|                    | Technique: sweep in a figure-8 pattern   |
|                    | through vegetation; empty net into a     |
|                    | killing jar or collecting bag after      |
|                    | every 10-20 sweeps.                      |
+--------------------+------------------------------------------+
| Beating tray       | Arboreal insects on trees and shrubs.    |
|                    | Hold a white sheet or tray under a       |
|                    | branch; strike the branch sharply 3-5    |
|                    | times; collect dislodged insects with    |
|                    | an aspirator or forceps.                 |
+--------------------+------------------------------------------+
| Pitfall trap       | Ground-dwelling insects (beetles,        |
|                    | ants, crickets). Bury a cup flush with   |
|                    | the soil surface. Add a rain cover.      |
|                    | Check every 24-48 hours. Use propylene   |
|                    | glycol as preservative (non-toxic to     |
|                    | mammals; do not use ethylene glycol).    |
+--------------------+------------------------------------------+
| Light trap         | Nocturnal flying insects (moths, many    |
|                    | beetles, lacewings). Use a white sheet   |
|                    | illuminated by a mercury vapor or UV     |
|                    | light. Operate from dusk to midnight     |
|                    | or dawn. Most effective on warm, humid,  |
|                    | moonless nights.                         |
+--------------------+------------------------------------------+
| Malaise trap       | Flying insects, especially Hymenoptera   |
|                    | and Diptera. A tent-like mesh barrier    |
|                    | that intercepts insects in flight;       |
|                    | they walk upward into a collecting head  |
|                    | containing preservative. Runs            |
|                    | continuously; check weekly.              |
+--------------------+------------------------------------------+
| Aspirator (pooter) | Small, delicate insects that cannot be   |
|                    | handled with forceps. Suck the insect    |
|                    | into a vial through a tube (a mesh      |
|                    | filter prevents inhalation). Use only    |
|                    | mouth-operated aspirators with a filter. |
+--------------------+------------------------------------------+
| Pan trap           | Pollinators and small flying insects.    |
|                    | Colored bowls (yellow, white, blue)      |
|                    | filled with soapy water. Place at        |
|                    | vegetation height. The soap breaks       |
|                    | surface tension; insects fall in and     |
|                    | drown. Check every 24-48 hours.          |
+--------------------+------------------------------------------+
| Hand collection    | Large, slow, or sessile insects.         |
|                    | Pick directly with forceps or fingers.   |
|                    | Useful for bark-dwelling beetles,        |
|                    | caterpillars on host plants, aquatic     |
|                    | larvae under rocks.                      |
+--------------------+------------------------------------------+

Expected: One or more collection methods selected based on target taxa and habitat, with equipment assembled and ready before entering the field.

On failure: If the intended method is not yielding specimens (e.g., sweep netting in heavy rain), switch to an alternative method. Light trapping requires specific weather conditions — warm, humid, still, moonless nights are optimal. If conditions are poor, reschedule rather than running traps inefficiently.

Step 3: Dispatch Specimens Humanely

Kill collected insects as quickly and humanely as possible. Prolonged distress damages specimens (broken legs, lost scales) and is ethically unacceptable.

Dispatch Methods:
+--------------------+------------------------------------------+
| Method             | Procedure and Notes                      |
+--------------------+------------------------------------------+
| Ethyl acetate      | Place a wad of absorbent material        |
| killing jar        | (plaster of Paris or tissue) in the      |
|                    | bottom of a wide-mouth jar. Saturate     |
|                    | with ethyl acetate. Place insects in     |
|                    | the jar; death occurs within 1-5        |
|                    | minutes for most species.                |
|                    | Caution: ethyl acetate is flammable and  |
|                    | an irritant. Use in well-ventilated     |
|                    | areas. Do not inhale.                    |
+--------------------+------------------------------------------+
| Freezing           | Place live insects in a container in a   |
|                    | freezer at -20C for 24 hours. Suitable   |
|                    | for specimens brought back alive.        |
|                    | Produces well-relaxed specimens ideal    |
|                    | for pinning.                             |
+--------------------+------------------------------------------+
| Ethanol drowning   | Immerse directly in 70-95% ethanol.      |
|                    | Used for soft-bodied insects that will   |
|                    | be wet-preserved (larvae, aphids, small  |
|                    | Diptera). Not suitable for Lepidoptera   |
|                    | (destroys scales) or specimens intended  |
|                    | for dry pinning.                         |
+--------------------+------------------------------------------+

NEVER use:
- Cyanide jars (potassium cyanide) — extremely toxic to humans;
  obsolete in modern entomology
- Crushing or squeezing — destroys morphological features
- Prolonged suffocation — slow and damages specimens from struggling

Expected: Specimens dispatched quickly (within minutes) with minimal damage to morphological features. Lepidoptera kept separate to prevent scale loss from contact with other specimens.

On failure: If ethyl acetate is unavailable, freezing is the best alternative for most taxa. In the field without either, place specimens in individual vials or envelopes (for Lepidoptera, use glassine envelopes with wings folded) and freeze upon return. Do not leave live insects in a sealed container without a killing agent — they will damage themselves.

Step 4: Pin Specimens (Dry Preservation)

Pin each specimen through the correct location for its order. Proper pin placement is essential for both access to diagnostic features and long-term structural integrity.

Pin Placement by Order:
+--------------------+------------------------------------------+
| Order              | Pin Position                             |
+--------------------+------------------------------------------+
| Coleoptera         | Through the RIGHT ELYTRON (front wing    |
| (beetles)          | cover), approximately 1/3 from the       |
|                    | anterior edge, so the pin emerges        |
|                    | between the middle and hind legs.        |
+--------------------+------------------------------------------+
| Lepidoptera        | Through the CENTER OF THE THORAX         |
| (butterflies/moths)| (mesothorax), between the wing bases.    |
|                    | Wings must be spread on a spreading      |
|                    | board before the specimen dries.         |
+--------------------+------------------------------------------+
| Hymenoptera        | Through the RIGHT SIDE OF THE THORAX     |
| (bees/wasps/ants)  | (mesothorax), between the wing bases.    |
+--------------------+------------------------------------------+
| Diptera            | Through the RIGHT SIDE OF THE THORAX     |
| (flies)            | (mesothorax), between the wing bases.    |
+--------------------+------------------------------------------+
| Hemiptera          | Through the RIGHT SIDE OF THE            |
| (true bugs)        | SCUTELLUM (triangular plate between      |
|                    | wing bases), slightly to the right of    |
|                    | center.                                  |
+--------------------+------------------------------------------+
| Orthoptera         | Through the RIGHT SIDE OF THE            |
| (grasshoppers)     | PRONOTUM (just behind the head), to      |
|                    | the right of the midline.                |
+--------------------+------------------------------------------+
| Odonata            | Through the CENTER OF THE THORAX.        |
| (dragonflies)      | Wings must be spread. Alternatively,     |
|                    | store in glassine envelopes.             |
+--------------------+------------------------------------------+
| All other orders   | Through the RIGHT SIDE OF THE THORAX     |
|                    | unless order-specific guidance is        |
|                    | available.                               |
+--------------------+------------------------------------------+

Pin Selection:
- Standard entomological pins: stainless steel, sizes 0-7
- Size 3 (0.50mm) is the most commonly used general-purpose size
- Size 1-2 for small beetles and flies; size 4-5 for large beetles
- Specimens under 5mm: mount on a paper point (triangular card
  glued to a standard pin) rather than pinning directly

Pin Height:
- The specimen should sit approximately 2/3 up the pin (leaving
  room below for 2 labels and above for handling)
- Use a pinning block (stepped block with 3 heights) to ensure
  consistent specimen and label heights across the collection

Spreading Wings (Lepidoptera, Odonata):
1. Pin the specimen through the thorax
2. Place on the spreading board with the body in the groove
3. Use paper strips to hold wings in position
4. Adjust wings so the hind margin of the forewing is perpendicular
   to the body axis
5. Leave on the board for 3-7 days until completely dry
6. Remove paper strips carefully

Expected: Each specimen pinned through the correct position for its order, at the correct height on the pin, with wings spread where required (Lepidoptera, Odonata). Specimens allowed to dry fully before handling.

On failure: If a specimen is too dry and brittle to pin (legs snapping, wings cracking), it needs relaxing first. Place the specimen in a relaxing chamber (a sealed container with damp sand or paper towels and a few drops of phenol to prevent mold) for 24-48 hours until limbs are pliable. If a pin is placed in the wrong position, it is better to carefully re-pin while the specimen is still fresh than to leave it incorrectly mounted.

Step 5: Preserve in Ethanol (Wet Preservation)

Soft-bodied specimens that would shrivel or distort if dried must be preserved in liquid.

Wet Preservation Protocol:
+--------------------+------------------------------------------+
| Category           | Procedure                                |
+--------------------+------------------------------------------+
| Preservative       | 70-80% ethanol for morphological study.  |
|                    | 95-100% ethanol for DNA-grade            |
|                    | preservation (change ethanol after 24    |
|                    | hours to remove dilution from body       |
|                    | fluids).                                 |
+--------------------+------------------------------------------+
| Suitable specimens | Larvae (caterpillars, grubs, maggots),   |
|                    | soft-bodied adults (aphids, termites,    |
|                    | some small Diptera), aquatic insects,    |
|                    | immature stages (nymphs, pupae)          |
+--------------------+------------------------------------------+
| Containers         | Glass vials with screw caps or           |
|                    | polyethylene snap-cap vials. Avoid       |
|                    | rubber stoppers (ethanol dissolves       |
|                    | them). Label goes INSIDE the vial.       |
+--------------------+------------------------------------------+
| Fluid ratio        | At least 3 parts preservative to 1 part  |
|                    | specimen volume. Too little fluid        |
|                    | results in poor preservation.            |
+--------------------+------------------------------------------+
| Long-term storage  | Check fluid levels every 6-12 months.    |
|                    | Ethanol evaporates even through sealed   |
|                    | caps. Top up as needed. Store in a cool, |
|                    | dark location.                           |
+--------------------+------------------------------------------+

Do NOT use:
- Formaldehyde/formalin for routine insect preservation (destroys DNA,
  poses health risks, requires special disposal). Some historical
  collections used it; modern practice strongly discourages it.
- Isopropanol as a substitute — it causes excessive hardening and
  color loss compared to ethanol.

Expected: Soft-bodied specimens preserved in 70-80% ethanol (or 95%+ for DNA work) in labeled vials with sufficient fluid volume.

On failure: If ethanol is unavailable in the field, specimens can be temporarily stored in high-proof clear spirits (vodka, Everclear) as an emergency measure. Transfer to laboratory-grade ethanol as soon as possible. If specimens have been stored too long in weak preservative and show decomposition, they may still be identifiable but will be unsuitable for molecular work.

Step 6: Label Every Specimen

Every specimen must carry labels providing the minimum data needed for scientific use. An unlabeled specimen has no scientific value.

Labeling Standards:

LABEL 1 (Locality label — placed closest to the specimen on the pin):
  Line 1: Country, State/Province
  Line 2: Specific locality (e.g., "3 km NE of Oakville, Elm Creek trail")
  Line 3: Latitude/Longitude (decimal degrees preferred)
  Line 4: Elevation (meters above sea level)
  Line 5: Date (e.g., 15.vi.2026 or 15-Jun-2026)
  Line 6: Collector name (e.g., "leg. P. Thoss")

LABEL 2 (Habitat/method label — below the locality label):
  Line 1: Habitat (e.g., "deciduous forest, oak canopy")
  Line 2: Collection method (e.g., "sweep net" or "light trap")
  Line 3: Additional ecological data if relevant

LABEL 3 (Determination label — lowest on the pin, added when identified):
  Line 1: Order Family
  Line 2: Genus species Author, Year
  Line 3: "det. [identifier name], [year]"

Label Format Rules:
- Use archival-quality paper (acid-free, resistant to fumigant chemicals)
- Print labels using a laser printer (inkjet fades; handwriting smudges)
- Labels should be small (approximately 13mm x 8mm) — do not obscure
  the specimen
- For wet specimens, the label goes INSIDE the vial on acid-free paper
  written in pencil or printed with a laser printer (ink dissolves in
  ethanol; pencil graphite does not)
- Pin labels below the specimen using the pinning block for consistent
  heights

Expected: Every specimen carries at minimum a locality label with country, locality, coordinates, date, and collector. Wet specimens have the same data on an internal label written in pencil or laser-printed.

On failure: If GPS coordinates were not recorded in the field, estimate them from a map using the locality description. If the date is uncertain, record the best estimate and mark it with a question mark. A specimen with approximate data is far more valuable than one with no label at all. Never move a label from one specimen to another.

Step 7: Store and Protect the Collection

Proper storage protects specimens from physical damage, pests, and environmental degradation.

Dry Collection Storage:
+--------------------+------------------------------------------+
| Component          | Standard                                 |
+--------------------+------------------------------------------+
| Unit trays         | Cardboard or plastic trays with foam     |
|                    | bottoms (plastazote preferred — pinnable |
|                    | and chemically inert). Specimens pinned  |
|                    | into the foam in organized rows.         |
+--------------------+------------------------------------------+
| Drawers            | Tight-fitting drawers that exclude dust  |
|                    | and pests. Glass-topped drawers allow    |
|                    | viewing without opening.                 |
+--------------------+------------------------------------------+
| Cabinets           | Steel cabinets with tight seals.         |
|                    | Compressed-air gaskets are ideal.        |
+--------------------+------------------------------------------+
| Pest management    | Place pest strips (dichlorvos/DDVP) or   |
|                    | naphthalene/paradichlorobenzene crystals  |
|                    | in each drawer. Check and replace every  |
|                    | 6 months. Museum beetle (Anthrenus) and  |
|                    | book lice (Psocoptera) are the primary   |
|                    | pests — a single infestation can destroy |
|                    | an entire drawer.                        |
+--------------------+------------------------------------------+
| Climate control    | Target: 40-50% relative humidity,        |
|                    | 18-22C temperature. Fluctuations cause   |
|                    | expansion/contraction damage. Avoid      |
|                    | direct sunlight (fades color).           |
+--------------------+------------------------------------------+

Wet Collection Storage:
- Store vials upright in racks or jars
- Check fluid levels every 6-12 months; top up with fresh ethanol
- Store in a cool, dark, well-ventilated area (ethanol fumes)
- Keep away from ignition sources (ethanol is flammable)
- For long-term storage, use screw-cap glass vials; snap-cap
  plastic vials allow more evaporation

Expected: Dry specimens stored in sealed drawers with pest deterrents. Wet specimens stored upright with adequate ethanol levels. Storage area has stable temperature and humidity.

On failure: If proper museum storage is not available, store pinned specimens in airtight plastic containers (tackle boxes, Tupperware) with foam inserts and pest deterrent. This is adequate for personal collections and short-term storage. For long-term preservation of scientifically valuable specimens, deposit them in a recognized museum or university collection.

Step 8: Curate and Enter into Database

Maintain the collection as a living scientific resource through systematic curation and data management.

Curation Tasks:
+--------------------+------------------------------------------+
| Task               | Frequency                                |
+--------------------+------------------------------------------+
| Pest inspection    | Every 3-6 months. Look for frass (fine   |
|                    | powder under specimens), cast skins,     |
|                    | or live pests in drawers.                |
+--------------------+------------------------------------------+
| Fumigant refresh   | Every 6 months. Replace pest strips or   |
|                    | crystals. Ensure drawers seal tightly.   |
+--------------------+------------------------------------------+
| Ethanol top-up     | Every 6-12 months for wet collections.   |
+--------------------+------------------------------------------+
| Repair             | Re-pin loose specimens. Re-glue detached |
|                    | appendages (use water-soluble PVA glue). |
|                    | Replace damaged labels.                  |
+--------------------+------------------------------------------+
| Identification     | Send unidentified specimens to           |
| updates            | specialists. Update determination labels |
|                    | as IDs are returned — never remove old   |
|                    | determination labels; add new ones below.|
+--------------------+------------------------------------------+

Database Entry (minimum fields):
- Catalog number (unique identifier for each specimen)
- Taxon (order, family, genus, species)
- Locality (country, state, specific location, coordinates)
- Date of collection
- Collector
- Collection method
- Determiner and determination date
- Storage location (cabinet, drawer, row, position)
- Preservation type (pinned, ethanol, slide-mounted, point-mounted)

Database Standards:
- Use Darwin Core format for interoperability with global databases
  (GBIF, iDigBio)
- Record coordinates in decimal degrees (WGS84 datum)
- Use ISO 8601 date format (YYYY-MM-DD) in databases
- Assign a unique catalog number to every specimen, even if unidentified

Expected: All specimens cataloged in a database with unique identifiers, taxonomy, locality, date, collector, and storage location. Collection is on a regular inspection and maintenance schedule.

On failure: If a full database is not feasible, maintain at minimum a handwritten catalog or spreadsheet with catalog numbers corresponding to specimens. The catalog number links the specimen to its data — without it, the specimen and its data become disconnected if labels are lost. Even a simple numbered list is better than no catalog at all.

Validation

• Legal requirements were verified and permits obtained before collecting
• Collection methods were appropriate for the target taxa and habitat
• Specimens were dispatched humanely and promptly
• Dry specimens were pinned through the correct position for their order
• Lepidoptera and Odonata had wings properly spread before drying
• Soft-bodied specimens were preserved in 70-80% ethanol
• Every specimen carries a locality label with date, location, coordinates, and collector
• Wet specimen labels are written in pencil or laser-printed and placed inside the vial
• Storage includes pest deterrents and stable environmental conditions
• Specimens are cataloged in a database or notebook with unique identifiers

Common Pitfalls

• Collecting without permits: A specimen collected illegally cannot be used in published research, deposited in a museum, or transferred across borders. Always obtain authorization first
• Over-collecting: Taking more specimens than needed depletes populations without scientific benefit. Collect the minimum required for identification (often 5-10 individuals per morphospecies per site)
• Mixing specimens from different sites in one container: This makes locality data uncertain for all specimens in the batch. Keep each collecting event in a separate container with its own temporary label
• Using the wrong pin position: Pinning a beetle through the center of the thorax instead of the right elytron obscures ventral diagnostic features. Always check the order-specific pin position
• Ethanol concentration too low for DNA work: Specimens for molecular analysis require 95%+ ethanol with a change after 24 hours to remove body fluid dilution. Standard 70% ethanol preserves morphology but degrades DNA over time
• Forgetting to label wet specimens internally: A label taped to the outside of a vial can detach. The label inside the vial is the permanent record. Always place a pencil-written or laser-printed label inside with the specimen
• Neglecting pest management: Dermestid beetles (museum beetles) can destroy an entire drawer of specimens in weeks. Regular pest monitoring and fumigant replacement are not optional for any collection stored longer than a few months

Related Skills

• identify-insect — morphological identification of collected specimens using dichotomous keys, wing venation, mouthparts, and antennae
• document-insect-sighting — photographic and contextual documentation of sightings that may supplement or replace physical collecting
• observe-insect-behavior — behavioral observation protocols for live insects before or instead of collecting
• survey-insect-population — systematic population surveys that typically require specimen collection for identification and voucher purposes