1. Dissemination of supplies to community scientists

1. Carefully review and gather the full list of collection-related supplies needed by consulting the complete Table of Materials.
2. If sample collection will take place at multiple locations and/or by multiple individuals/teams, gather and organize all supplies needed into separate deployable units (Figure 1 and Figure 2).
3. Transport supplies (deployable units) to community scientists or other personnel responsible for field collection.
4. If personnel are not local, carefully pack supplies (each deployable unit) into a separate cardboard shipping box with a complete shipping label and ship.
   ​NOTE: Expedited shipping is not required at this stage.

2. Community scientist collection preparation

1. Upon receipt of collection supplies, including the collection tacklebox, carefully review the laminated supply list and conduct a full inventory. Notify the project leader if any supplies are missing.
2. Prefill 1.5 mL microcentrifuge tubes with 180 µL of lysis buffer, apply labels with a preprinted unique ID label to each microcentrifuge tube, and place all tubes in the 64-well microcentrifuge tubes storage box. Firmly secure the lid after loading.
   NOTE: If label printers are not available, apply unique ID numbers to the side and lid of each vial using an ethanol-proof marker.
3. Ensure all digital equipment (e.g., smartphone or camera) is fully charged, and any spare batteries are packed.
4. Partially fill a small cooler with ice for field storage and local transportation of the collected samples.
5. Pack all collection supplies into the collection tacklebox or similar sturdy, weatherproof container for safe transport and consolidated storage.
6. Review the nondestructive genetic sample collection protocol in detail prior to heading into the field.
   NOTE: Use the laminated and condensed, illustrated protocol for additional guidance in the field (Supplemental Figure S1 and Supplemental Figure S2).

3. Sample collection in the field

1. Upon arriving at the field site, use a pencil or all-weather pen to record in the weatherproof field notebook the time of day, date, overall property name (e.g., Apalachicola National Forest), specific field site location name or description, and GPS reading if available, and the full name and roles of all persons present.
2. Locate a suitable habitat with the presence of larval host plant species specific to the target butterfly.
   NOTE: Use care to avoid or minimize impact to sensitive habitats, plant populations, and wildlife. In addition, be sure to secure all appropriate landowner permissions and/or permits prior to accessing a site and sample collection events.
3. Using a smartphone or camera, take detailed photographs of all field sites, sample collection locations, host plants, and any other information that may be relevant to the project. Use smartphones or other cameras that record GPS coordinates.
   NOTE: Photo Geotagging needs to be enabled on all smartphones.
4. Comprehensively search all the larval host plant parts, such as leaves, flower buds, flowers, or developing fruit, known to be selected by ovipositing (egg-laying) adult female butterflies for hatched eggs. For most Lycaenidae, look for white, hatched eggs with a distinct hole in the center resembling a doughnut from which the neonate larva emerged (Figure 3). Look for unhatched eggs that are somewhat darker in color, often green or bluish, and will be completely intact without a hole in the middle (Figure 4). Use a hand lens or other magnifying device to inspect each egg closely.
5. Once a hatched egg has been located, put nitrile gloves on both hands.
6. Using clean, sterile, pointed forceps, grab and gently pull the hatched egg off the host plant and place it directly into a labeled microcentrifuge tube prefilled with lysis buffer taken from the 64-well storage box.
   NOTE: Some host plant carryover material (smaller than 15 mm in diameter) is acceptable and normal during collection.
7. Collect at a minimum a total of 5 samples per host plant patch/site (each containing 1-20 hatched eggs), aiming for >50 eggs total at a location if available.
   NOTE: This will help ensure at least some tissue is collected at every sample plant/patch and increase the chances of detecting DNA (personal observation).
8. After each egg collection, carefully clean the forceps tips by dipping them in a vial of 95% ethanol or by dousing with 95% ethanol from a squeeze bottle or by using alcohol wipes.
   NOTE: This will help minimize tissue carryover between sampling events.
9. If available, collect several hatched eggs (1-20 eggs) from multiple plants in the same host patch into a single microcentrifuge tube and firmly close the lid. For butterfly species utilizing larger herbaceous or woody host species, collect multiple eggs from different locations on the same plant if host patches are limited.
   NOTE: Plants are in the same host patch if their leaves touch one another. If there is a noticeable physical separation between plants or patches, this should be considered a different sample. If collecting another tissue type, such as larval exuviae or a single leg, place only a single leg, leg fragment, or larval exuvia into a microcentrifuge tube (one sample per individual).
10. Make sure that all collected material is fully submerged in the lysis buffer within each 1.5 mL microcentrifuge tube. Tap the bottom of the tube in question on a hard surface to resubmerge any samples if needed.
11. Wipe the forceps to dry with a clean disposable lab wipe.
    NOTE: Careful forceps cleaning is essential to avoid cross contamination between samples.
12. When collecting a new sample, discard used nitrile gloves and replace them with a clean pair.
13. In a weatherproof field notebook, use a pencil or all-weather pen to record the unique ID label assigned from the microcentrifuge tube along with the type of sample (e.g., eggs, larval exuviae, or leg), the approximate number of hatched eggs, and collection information such as collector name(s), date, location, host plant species, and any additional notes (Figure 2).
14. Place the closed microcentrifuge tube with egg debris sample back in the 64-well microcentrifuge storage box.
15. Maintain the 64-well microcentrifuge storage box in a cooler with ice while in the field.
16. Maintain all other collection supplies in the collection tacklebox while in the field for safe and consolidated storage and transport between sites.

4. When field collection is complete

1. Ensure all microcentrifuge tubes containing samples are in the 64-well microcentrifuge storage box in a cooler with ice for transport.
2. Place all field collection supplies back in the collection tacklebox.
3. Transport all samples back to the office or laboratory and carefully double-check each microcentrifuge tube to ensure that all sample material is completely submerged in lysis buffer.
4. Place the 64-well microcentrifuge storage box with samples in a freezer until shipment or processing.
   NOTE: An average commercial freezer of-18 °C is acceptable for short-term storage.
5. Carefully assess all supplies in the collection toolbox and replace any as needed.
   NOTE: This is particularly important if multiple field collection events are scheduled.
6. Store the collection tacklebox in a secure location until the next field collection event.
7. Download all digital images and ensure all are backed up securely on a server or cloud-based storage system.
8. Scan or photograph the original weatherproof, field notebook pages, or field data sheets containing collection data until all information can be entered into a project spreadsheet or database.

5. Submitting samples and data

1. Remove all 64-well microcentrifuge storage boxes with samples from the freezer.
2. Carefully package the 64-well microcentrifuge storage boxes with samples and the field notebook or field data sheets in a standard shipping box, attach the provided shipping label with the original sender's account number, and send via express carrier-guaranteed, overnight, next-day delivery to the project director.
3. Email the package tracking number and a copy of the scanned notebook pages or field data sheets to the project director.

6. DNA extraction

1. Once the 64-well microcentrifuge storage boxes are received, store them at -20 °C for the preservation of DNA in samples until ready for DNA extraction.
2. In the lab, extract DNA by grinding insect tissue stored in lysis buffer after thawing from the -20 °C. Add 20 µL of Proteinase K and let the sample soak overnight at 56 °C in a heated incubator for no more than 24 h.
3. Add the appropriate cleaning and washing buffers, per the specific manufacturer's recommendation¹³.
4. Transfer the sample suspended in buffer into a spin column attached to a 2 mL collection vial.
5. Spin down at 6,021 × g for 60 s using a centrifuge. Add the appropriate washing buffers and spin down appropriately.
6. Release bound DNA using elusion buffer (30 µL) and spin down the sample into a fresh 1.5 mL microcentrifuge tube. Store at -20 °C.
   ​NOTE: Proceed to sequencing if the DNA concentration exceeds 0.010 ng/mL. See Figure 5 for DNA concentration by tissue type.

7. Data analysis of DNA sequences

1. Trim or edit low-quality base calls in resulting sequences.
2. Query sequences against public databases for confirmation of species identification.
3. Align sequences to each other for comparison of differences between individuals.