trapping system seems to be a relatively inexpensive and time savingtechnique for sampling terrapins in an undersampled portionof their range.Acknowledgments.—We thank D. Nelson for sharing his knowledgeof Diamondback Terrapin nesting habitat in Alabama. We also thank theUniversity of South Alabama Biology Department for logistical support.We thank B. Jones, B. Gill, and A. Coleman for their assistance withconstruction of the drift fence and pitfalls. We are grateful to the GrandBay National Estuarine Research Reserve staff and Grand Bay US Fishand Wildlife Refuge Manager P. Dixon who provided detailed site descriptions,maps, and aerial photography. Funding for this project wasprovided by the Alabama Center for Estuarine Studies through a grant toD. Nelson. The University of South Alabama Institutional Animal Careand Use Committee approved animal care guidelines. Terrapins were capturedwith permission of the Alabama Department of Conservation andNatural Resources.LITERATURE CITEDCHRISTIANSEN, J. L., AND T. VANDEWALLE. 2000. Effectiveness of three traptypes in drift fence surveys. Herpetol. Rev. 31:158–160.CONGDON, J. D., G. L. BREITENBACH, R. C. VAN LOBEN SELS, AND D. W.Tinkle. 1987. Reproduction and nesting ecology of snapping turtles(Chelydra serpentina) in southeastern Michigan. Herpetologica 43:39–54.ERNST, C. H., J. E. LOVICH, AND R. W. BARBOUR. 1994. Turtles of the UnitedStates and Canada. Smithsonian Institution Press, Washington andLondon. 578 pp.FEINBERG, J. A., AND R. L. BURKE. 2003. Nesting ecology and predation ofdiamondback terrapins, Malaclemys terrapin, at Gateway NationalRecreation Area, New York. J. Herpetol. 37:517–526.GIBBONS, J. W., J. L. GREENE, AND J. D. CONGDON. 1983. Drought-relatedresponses of aquatic turtle populations. J. Herpetol. 17:242–246.NELSON, D. H., AND K. R. MARION. 2004. Mississippi diamondback terrapinMalaclemys terrapin pileata. In R. E. Mirarchi, M. A. Bailey, T. M.Haggerty, and T. L. Best (eds.), Alabama Wildlife. Volume 3. ImperiledAmphibians, Reptiles, Bird, and Mammals. The University of AlabamaPress, Tuscaloosa, Alabama.––––––, T. WIBBELS, K. R. MARION, AND J. DINDO. 2005. Annual report:survey of diamondback terrapin populations in Alabama estuaries.Unpubl. report, Alabama Center for Estuarine Studies.ROOSENBERG, W. M. 1996. Maternal condition and nest site choice: analternative for the maintenance of environmental sex determination?Amer. Zool. 36:157–168.––––––, AND A. E. DUNHAM. 1997. Allocation of reproductive output: eggandclutch-size variation in the diamondback terrapin. Copeia 1997:290–297.TUCKER, J. K. 2000. Body size and migration of hatchling turtles: interandintraspecific comparisons. J. Herpetol. 34:541–546.WOOD, R. C. 1997. The impact of commercial crab traps on northern diamondbackterrapins, Malaclemys terrapin terrapin. Proceedings: Conservation,Restoration, and Management of Tortoises and Turtles—AnInternational Conference, pp. 21–27.<strong>Herpetological</strong> <strong>Review</strong>, 2008, 39(2), 190–191.© 2008 by Society for the Study of Amphibians and ReptilesUse of Traditional Turtle Marking to Obtain DNAfor Population StudiesPATRICK J. DAWESCOLLEEN S. SINCLAIR*andRICHARD A. SEIGELDepartment of Biological Sciences, Towson University8000 York Road, Towson, Maryland 21252, USA*Corresponding author; e-mail: csinclair@towson.eduGenetic analysis has been applied extensively to studies of wildlifepopulations to examine population diversity, gene flow, inbreedingdepression, source-sink dynamics, and extinctionrecolonizationfrequencies (Hedrick and Kalinowski 2000; Jehleand Arntzen 2002). Blood or tissue samples and buccal swabs arethe common source of DNA for most genetic studies. In chelonians,blood samples are acquired by drawing blood from the tail,leg, or neck (Avery and Vitt 1984; Jacobson et al. 1992; Rosskopf1982). Although effective, obtaining blood samples is invasive,sometimes difficult to accomplish, and possibly stressful to theturtle. However, alternative methods have also had serious drawbacks,including a protocol using shell samples that required suchlarge amounts of bone that either a deceased animal was neededor the animal had to be sacrificed (Hsieh et al. 2006).In this paper, we describe a method of obtaining tissue for geneticstudies that makes use of the traditional marking techniquesfor turtles, i.e., drilling or notching the marginal scutes (Cagle 1939;Ernst et al. 1974; Mockford et al. 1999). The drill shavings producedduring marking are used as the source of DNA for geneticanalysis instead of being thrown away thereby eliminating the invasiveand stressful procedure of blood extraction and increasingthe speed with which the samples can be taken.Materials and Methods.—All samples collected came from gophertortoises at the Kennedy Space Center (Brevard and VolusiaCounties, Florida, USA) where mark-recapture studies have beenconducted for over 30 years (Pike et al. 2005). Tortoises collectedwere examined for previous marks and mass and length measurementswere recorded (Pike et al. 2005). While wearing sterilegloves, 100% ethanol was used to swab the scute area to be drilledin order minimize contamination of the sample. A 1/8 th inch (3.17mm) drill bit was used to drill holes in scutes of unmarked tortoises,while a larger bit was used to drill holes in scutes of previouslymarked individuals. Filter paper was placed under the scutearea where the hole was drilled to catch the drill shavings duringthe marking process. Drill shavings from one or two holes wereenough to facilitate genomic DNA extraction. After drilling, theshavings were placed in a sterile 15 ml polypropylene tube, andstored at ambient temperature. After a tortoise was marked, thedrill bit was cleaned by brushing with a firm toothbrush dipped in100% ethanol. The drill bit was then dipped in 100% ethanol andflamed to sterilize. (Note: Isopropyl alcohol could be substitutedfor ethanol.)The extraction process used two 5/8 th inch (15.88 mm) hex bolts190 <strong>Herpetological</strong> <strong>Review</strong> 39(2), 2008
and a matching nut. Prior to use, the threaded end of the boltswere ground flat to provide an even grinding surface to maximizethe pulverization of the drill shavings (Thomas and Moore 1997).The nuts and bolts were then wrapped in aluminum foil and sterilizedin an autoclave. The nut was partially threaded on to one boltcreating a small cup that was then filled with approximately 0.1 gof drill shavings. The second bolt was added to make a sealedchamber encapsulating the drill shavings (Thomas and Moore1997). The bolt assembly was placed in liquid nitrogen for 30seconds to one minute (Thomas and Moore 1997). Upon removalfrom the liquid nitrogen, the sample was pulverized by simultaneouslytwisting both bolts together. The bolt assembly was tightenedand loosened several times and tapped on the hard surface toassure the sample was uniformly pulverized (Thomas and Moore1997). The bolt assembly was then carefully dismantled over apiece of filter paper to collect the powder and facilitate transfer toa 1.5 ml microcentrifuge tube.The powdered drill shavings were decalcified in 500 µl of 0.5M pH 8.0 EDTA at 37ºC while shaking at 225 rpm until the pelletshad broken down, (approximately three to five days) following amodified protocol for the Qiagen DNeasy Blood and Tissue kit(Qiagen, Valencia, California) (Qiagen 2006). The decalcificationstep is critical since the cells containing DNA must be freed fromthe calcified matrix in order for the extraction to be successful.The samples were centrifuged at 13,000 rpm to pellet and washedthree times with sterile deionized water to remove ions that hadaccumulated during the decalcification process. Decalcifiedsamples were then processed using a Qiagen DNeasy Blood andTissue kit following the modified protocol above.Results.—A total of 0.1 g of drill shavings yielded enough DNAfor multiple genetic analyses. Total DNA yields ranged from 110to 4650 ng. The high molecular weight DNA produced with thismethod has been verified by ultraviolet spectrophotometry andPCR. Ratios of A260/A280 measurements ranged from 1.6 to 2.0.PCR amplifications with seven species-specific microsatelliteprimers produced strong, clear bands in >91% of the samples tested.Discussion.—Our results show that DNA can be obtained froma standard method of marking turtles. By refining and combiningexisting techniques, we have developed a protocol that requireslesser amounts of shell material and minimizes the invasive procedureswhen compared to currently published techniques. Thedrilling or filing of the marginal scutes has been observed to showno signs of physical pain in the animals (Gibbons 1968). Pike etal. (2005) also noted that handling and drilling stress wore offquickly enough to have no discernable effect on recapture rates,demonstrating that drill marking has little detrimental effect ontortoises. Mockford et al. (1999) described a similar protocol forDNA extraction from freshwater turtle hatchlings; however it isimportant to note that the shell material was not ossified at thetime of removal making the DNA extraction process less problematic.Our technique provides the basis to easily gather and processgenetic material from ossified shell to examine chelonian geneticdiversity and long-term viability. A better understanding of thepopulation structure and effective populations of these long-livedand slow reproducing animals is necessary to properly formulatemanagement strategies for these animals (Gibbons et al. 2000; Scottand Seigel 1992). Our protocol uses a waste product of a commonmarking technique to obtain high-quality DNA allowing for theaddition of genetic analysis to ongoing mark-recapture studies.Our technique enables non-invasive sampling of a population toget DNA samples of comparable quality to those obtained withmore invasive methods.Acknowledgments.—Special thanks go to R. Bolt for her constant andgracious help with this project. Much of what we have done could nothave been accomplished without her assistance. Thanks also go to S. Weissand P. Cain for their help in locating tortoises for this study. We wouldalso like to thank T. Crabill for her advice on bucket trap placement and J.Sinclair for his valuable comments on this manuscript. We are also gratefulto R. Hinkle of Dynamac and J. Stiner of the National Park Service forfinancial support. We thank personnel from the Merritt Island NationalWildlife Refuge (especially M. Epstein and M. Legare) for providingpermits to conduct this study. We also thank the Canaveral National Seashore(J. Stiner) for logistical support and special use permits. All procedureswere approved by the NASA Animal Care and Use Permit #GRD-06-042 with R. Bolt as the point of contact.LITERATURE CITEDAVERY, H. R., AND L. J. VITT. 1984. How to get blood from a turtle. Copeia1984:209–210.CAGLE, F. R. 1939. A system of marking turtles for future identification.Copeia 1939:170–173.ERNST, C. H., R. W. BARBOUR, AND M. F. HERSHEY. 1974. A new codingsystem for hard shelled turtles. Trans. Kentucky Acad. Sci. 35:27–28.GIBBONS, J. W. 1968. Population structure and survivorship in the paintedturtle, Chrysemys picta. Copeia 1968:360–368.––––––, D. E. SCOTT, T. J. RYAN, K. A. BUHLMANN, T. D. TUBERVILLE, B. S.METTS, J. L. GREEN, T. MILLS, Y. LEIDEN, S. POPPY, AND C. T. WINNE.2000. The global decline of reptiles, dèjá vu amphibians. Bioscience50:653–666.HEDRICK, P. W., AND S. T. KALINOWSKI. 2000. Inbreeding depression inconservation biology. Annu. Rev. Ecol. Syst. 31:139–162.HSIEH, H.-M., L.-H. HUANG, L.-C. TSAI, C.-L. LIU, Y.-C. KUO, C.-T. HSIAO,A. LINACRE, AND J. C.-I. LEE. 2006. Species identification of Kachugatecta using the cytochrome b gene. J. Forensic Sci. 51:52–56.JACOBSON, E. R., J. SCHUMACHER, AND M. GREEN. 1992. Field and clinicaltechniques for sampling and handling blood for hematologic and selectedbiochemical determinations in the desert tortoise Xerobatesagassizii. Copeia 1992:237–241.JEHLE, R., AND J. W. ARNTZEN. 2002. Microsatellite markers in amphibianconservation genetics. Herpetol. J. 12:1–9.MOCKFORD, S. W., J. M. WRIGHT, M. SNYDER, AND T. B. HERMAN. 1999. Anon-destructive source of DNA from hatchling freshwater turtles foruse in PCR base assays. Herpetol. Rev. 30:148–149.PIKE, D. A., A. DINSMORE, T. CRABILL, R. B. SMITH, AND R. A. SEIGEL.2005. Short-term effects of handling and permanently marking gophertortoises (Gopherus polyphemus) on recapture rates and behavior.Appl. Herpetol. 2:139–147.QIAGEN. 2006. Purification of total DNA from compact animal bone usingDNeasy blood & tissue kit. http://www1.qiagen.com/literature/protocols/pdf/DY01.pdf.ROSSKOPF, W. J. 1982. Normal hemogram and blood chemistry values forCalifornia desert tortoises. Vet. Med./Small Anim. Clin. 77:85–87.SCOTT JR., N. J., AND R. A. SEIGEL. 1992. The management of amphibianand reptile populations: species priorities and methodological and theoreticalconstraints. In D. R. McCullough, and R. H. Barrett (eds.), Wildlife2001: Populations, pp. 343–368. Elsevier Applied Science, London.THOMAS, M. G., AND L. J. MOORE. 1997. Preparation of bone samples forDNA extraction: a nuts and bolts approach. BioTechniques 22:402.<strong>Herpetological</strong> <strong>Review</strong> 39(2), 2008 191
- Page 1 and 2:
HerpetologicalReviewVolume 39, Numb
- Page 3 and 4:
About Our Cover: Zonosaurus maramai
- Page 5 and 6:
Prey-specific Predatory Behavior in
- Page 7 and 8:
acid water treatment than in the co
- Page 10 and 11:
TABLE 1. Time-line history of croco
- Page 12 and 13:
The Reptile House at the Bronx Zoo
- Page 14 and 15: FIG. 6. A 3.9 m (12' 11 1 / 2") Ame
- Page 16 and 17: One of the earliest studies of croc
- Page 18 and 19: TABLE 2. Dimensions and water depth
- Page 20 and 21: we call it, is in flux.Forty years
- Page 22 and 23: Feb. 20-25. abstract.------. 1979.
- Page 24 and 25: yond current practices (Clarke 1972
- Page 26 and 27: poles (Pond 1 > 10,000, Pond 2 4,87
- Page 28 and 29: ------, R. MATHEWS, AND R. KINGSING
- Page 30 and 31: Herpetological Review, 2008, 39(2),
- Page 32 and 33: TABLE 2. Summary of running (includ
- Page 34 and 35: FIG. 2. Responses of adult Regal Ho
- Page 36 and 37: PIANKA, E. R., AND W. S. PARKER. 19
- Page 38 and 39: BUSTAMANTE, M. R. 2005. La cecilia
- Page 40 and 41: Fig. 3. Mean clutch size (number of
- Page 42 and 43: facilitated work in Thailand. I tha
- Page 44 and 45: preocular are not fused. The specim
- Page 46 and 47: FIG. 2A) Side view photo of Aechmea
- Page 48 and 49: 364.DUELLMAN, W. E. 1978. The biolo
- Page 50 and 51: incision, and placed one drop of Ba
- Page 52 and 53: 13 cm deep (e.g., Spea hammondii; M
- Page 54 and 55: FIG. 1. Medicine dropper (60 ml) wi
- Page 56 and 57: esearchers and Hellbenders, especia
- Page 58 and 59: FIG. 3. Relative success of traps p
- Page 60 and 61: data on Hellbender population struc
- Page 62 and 63: aits sometimes resulted in differen
- Page 66 and 67: AMPHIBIAN CHYTRIDIOMYCOSISGEOGRAPHI
- Page 68 and 69: TABLE 1. Prevalence of B. dendrobat
- Page 70 and 71: Conservation Status of United State
- Page 72 and 73: TABLE 1. Wood Frog (Rana sylvatica)
- Page 74 and 75: TABLE 1. Anurans that tested positi
- Page 76 and 77: is, on average, exposed to slightly
- Page 78 and 79: (10%) were dead but not obviously m
- Page 80 and 81: Submitted by CHRIS T. McALLISTER, D
- Page 82 and 83: FIG. 1. Oscillogram, spectrogram, a
- Page 84 and 85: FIG. 1. Adult Physalaemus cuvieri r
- Page 86 and 87: Répteis, Instituto Nacional de Pes
- Page 88 and 89: discovered 145 live hatchlings and
- Page 90 and 91: GRAPTEMYS GIBBONSI (Pascagoula Map
- Page 92 and 93: College, and the Joseph Moore Museu
- Page 94 and 95: FIG. 1. Common Ground Lizard (Ameiv
- Page 96 and 97: havior unavailable elsewhere. Here
- Page 98 and 99: 15% of predator mass, is typical fo
- Page 100 and 101: side the third burrow and began a f
- Page 102 and 103: We thank Arlington James and the st
- Page 104 and 105: mm) S. viridicornis in its mouth in
- Page 106 and 107: NECTURUS MACULOSUS (Common Mudpuppy
- Page 108 and 109: LITHOBATES CATESBEIANUS (American B
- Page 110 and 111: Research and Collections Center, 13
- Page 112 and 113: BRONCHOCELA VIETNAMENSIS (Vietnam L
- Page 114 and 115:
Oficina Regional Guaymas, Guaymas,
- Page 116 and 117:
MICRURUS TENER (Texas Coralsnake).
- Page 118 and 119:
declining in this recently discover
- Page 120 and 121:
80.7372°W). 02 November 2005. Stev
- Page 122 and 123:
this effort, 7% of the 10 × 10 km
- Page 124 and 125:
the knowledge of the group. The aut
- Page 126 and 127:
which is listed under “Rhodin, A.
- Page 128 and 129:
noting that Sphenomorphus bignelli
- Page 130 and 131:
256 Herpetological Review 39(2), 20
- Page 132:
ISSN 0018-084XThe Official News-Jou