The Geek in Question
Want to contact The Geek?
Drop me a line at tgiq.ce at gmail dot com!
Geeky Tweets
- @TransLink The 6:06 just showed up...better late than never. Hopefully the gps gets fixed, that was worrisome! 11 months ago
- @TransLink stop 59181...have the next two busses really been cancelled? No indication the 6:06 was cancelled for holidays two hours ago 11 months ago
- @HakaiInstitute twitter.com/docdez/status/… 1 year ago
| Blog: |
| The Bug Geek |
Topics: |
| Insects, Nature, Photography |
Flickr Photos
Want some Bug Geek swag? You’ve come to the right place!
BugShot 2012 Crowd-Funding
Goal: $1000 (registration and half of the travel expenses)
Raised: $800
YOU PEOPLE ARE SO AWESOME! Thank you!!!
Copyright
All photographs and text are my own, unless otherwise noted. All text and images appearing on www.thebuggeek.com © C. M. Ernst 2009-2013 and may not be used without prior permission. See "About the Photographs" to learn more.
Sounds like quite the project! Depending on what sort of DNA work you’re looking at doing (genomic vs mitochondrial COI), and the time available to you for working with collected samples, you might be able to use 95% EtOH and exchange the alcohol a couple of times throughout the 4-14 days. I’ve gotten fairly consistent success with genomic genes using 95% EtOH as long as I make sure the alcohol is changed on the return from my trip and the specimens are placed in at least a -20C freezer as soon as possible until I’m ready to process them. If you’re dealing with bulk samples then I would recommend changing the alcohol more frequently as alcohol forces the water out of the insect’s bodies, diluting the alcohol and decreasing the preservative effect. Good luck!
See, therein lies the problem, Morgan: what I WANT to do is set a bunch of traps and leave them, unattended and undisturbed for about 4 days at a time. The specimens would be collected after the 4 days and could be put into high-octane alcohol at that point… but we likely won’t have much in the way of freezer space (we’ll be in very remote areas) right away. My other issue is that 100 or 95% EtOH tend to embrittle (is that a word? If not, I’m declaring it a new word, I like it) some arthropods and cause the setae of others to fall out…all bad things for longer-term storage and especially ID. Methinks I may have to develop completely separate ADDITIONAL sampling protocol for the DNA component. Le sigh.
Bummer! I can tell you that I’ve had a hard time getting any results from traditional pan trap samples or even low EtOH% malaise traps, COI or otherwise, so if you do come up with a new technique that doesn’t allow the insects to rot in the field, I’d love to hear about it! Good luck!