http://lod.bco-dmo.org/id/dataset/732524
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dataset
Highest level of data collection, from a common set of sensors or instrumentation, usually within the same research project
Biological and Chemical Oceanography Data Management Office (BCO-DMO)
Unavailable
508-289-2009
WHOI MS#36
Woods Hole
MA
02543
USA
info@bco-dmo.org
http://www.bco-dmo.org
Monday - Friday 8:00am - 5:00pm
For questions regarding this resource, please contact BCO-DMO via the email address provided.
pointOfContact
2018-03-28
ISO 19115-2 Geographic Information - Metadata - Part 2: Extensions for Imagery and Gridded Data
ISO 19115-2:2009(E)
Location, weathering, bulk isotope, and 14C data for fossil seals from the western Ross Sea, Antarctica from from 2013-2014
2018-03-28
publication
2018-03-28
revision
Marine Biological Laboratory/Woods Hole Oceanographic Institution Library (MBLWHOI DLA)
2022-08-22
publication
https://doi.org/10.26008/1912/bco-dmo.732524.1
Brenda Hall
University of Maine
principalInvestigator
Paul L. Koch
University of California-Santa Cruz
principalInvestigator
Daniel P. Costa
University of California-Santa Cruz
principalInvestigator
A. Rus Hoelzel
Durham University
principalInvestigator
Biological and Chemical Oceanography Data Management Office (BCO-DMO)
Unavailable
508-289-2009
WHOI MS#36
Woods Hole
MA
02543
USA
info@bco-dmo.org
http://www.bco-dmo.org
Monday - Friday 8:00am - 5:00pm
For questions regarding this resource, please contact BCO-DMO via the email address provided.
publisher
Cite this dataset as: Hall, B., Koch, P. L., Costa, D. P., Hoelzel, A. R. (2022) Location, weathering, bulk isotope, and 14C data for fossil seals from the western Ross Sea, Antarctica from from 2013-2014. Biological and Chemical Oceanography Data Management Office (BCO-DMO). (Version 1) Version Date 2018-03-28 [if applicable, indicate subset used]. doi:10.26008/1912/bco-dmo.732524.1 [access date]
Location, weathering, bulk isotope, and 14C data for fossil seals from the western Ross Sea, Antarctica Dataset Description: <p><strong>These data are published and discussed in:</strong><br />
Brault, E. (2017). An Examination of the Ecological and Oceanographic Effects of Mid-to-Late Holocene Climate Changes on the Ross Sea Ecosystem. UC Santa Cruz. ProQuest ID: Brault_ucsc_0036E_11435. Merritt ID: ark:/13030/m5dg1n5d. Retrieved from&nbsp;<a href="https://escholarship.org/uc/item/99s5j3fk" target="_blank">https://escholarship.org/uc/item/99s5j3fk</a></p> Methods and Sampling: <p><strong>Sample collection:</strong><br />
Fossil seal samples were collected during the austral summers of 2005/06, 2006/07, 2012/13, and 2013/14 in Antarctica in the Dry Valleys and along the Victoria Land Coast (especially Inexpressible Island on Terra Nova Bay), Antarctica. Since this region experiences unusually dry and cold conditions, carcasses and bones are well-preserved, potentially for several thousand years, and therefore have unchanged isotopic compositions in most cases. The sampled species were crabeater, Weddell, leopard, and southern elephant seals. Latitude and longitude of each specimen was determined by GPS and recorded, and several photographs were taken of each specimen. Bone and carcass weathering states were determined. Several samples were gathered from the specimens. Most commonly, bone was collected, followed by skin and fur; nails, teeth, and whiskers were not frequently available for sampling, but taken when possible. Samples were collected with ethanol-cleaned tools, stored in Whirl-Pak bags, and refrigerated (~4 °C) when we returned from the field.</p>
<p><strong>Carcass and Bone Weathering:</strong><br />
For each specimen, we assessed the extent to which the carcass had been degraded by exposure, as well as the weathering state of exposed bone.</p>
<p>We assigned each specimen to one of the following Carcass Weathering Stages. These stages are modified from Barwick and Balham (1967):<br />
A&nbsp;= Complete.Fresh. Undamaged from wind erosion, no desiccation.<br />
B = Complete. Slightly weathered. Partial erosion of hair on exposed surfaces, cracks in skin exposing deeper tissues or bones in the flippers or cranium.<br />
C = Incomplete. Extensive erosion and exposure of bones of upward part of body (skull, ribs, limbs). Skeleton undamaged but soft tissues eroding between bony elements.<br />
D = Incomplete. Extensive erosion with regional destruction of bone and tissues. Vertebral column completely exposed and 40-50% tissue is destroyed.<br />
E = Very incomplete. &gt;50% of carcass is eroded. Vertebral column and cranium incomplete; limbs and rib cage becoming remnants. Difficult or impossible to identify species, sex, size.<br />
F = Fragments or isolated bones.</p>
<p>Bone Weathering Stages were determined on the most weathered bone from the carcass. Modified from Todd (1987).<br />
0 = unweathered and fatty.<br />
1 = unweathered, articular surfaces intact with no surface cracking.<br />
2 = articular surfaces intact with some surface cracking.<br />
3 = articular surfaces exhibit some deterioration, but &gt;50% of articular surface remains intact.<br />
4 = intact articular surface restricted to a few small "islands;" &lt;50% of articular surface remains intact.<br />
5 = no articular surface area remains intact.<br />
6 = bone severely deteriorated; large areas of fibrous bone exposed.<br />
7 = small weathered bone fragment or isolated tooth.</p>
<p><strong>Species identification:</strong><br />
When possible, species identification of each specimen was conducted in the field via examination of teeth or bones with features unique to the four pinniped species. Additionally, the team at the University of Durham in the United Kingdom extracted and analyzed DNA from many specimens, described below, to confirm or establish the species identification</p>
<p><strong>Sample preparation for bulk isotope analyses:</strong><br />
Preparation of bone samples was based on established procedures and by preliminary method testing in the lab (DeNiro 1987, Ambrose 1990). Bone fragments (50 -100 mg) were weighed into a vial (BD Falcon 15 mL centrifuge tubes, polypropylene) and acidified (to remove bone mineral, sedimentary carbonates, and fulvic acids) by the addition of 5 mL HCl (0.5 M) at room temperature. The acid was removed approximately three days later. If the samples did not appear completely decalcified (i.e., remains inflexible), a fresh aliquot of acid was added every 24 hours until the bone was decalcified, leaving behind bone collagen. Upon decalcification, the collagen was rinsed five times with Milli-Q water (Thermo Fisher Scientific, Inc.), neutralizing the sample, and 5 mL NaOH (0.1 M) was added to the samples, which were then kept at room temperature, further purifying the bone collagen by removing humic acids. A fresh aliquot of 0.1 M NaOH was added to the sample every 24 hours until the sample was nearly white. Again, the material was rinsed five times with Milli-Q water; then, it was refrigerated until the lipid extraction procedure. Lipids were removed via an accelerated solvent extraction with 100% petroleum ether (Dionex ASE 200 Accelerated Solvent Extractor: 1500 psi; 60°C; 3 cycles).</p>
<p>Bone was the most common sample type available. As it integrates diet over the largest period among the sample types collected (i.e., much of the animal’s lifespan), we analyzed bone from each specimen when available (<em>n</em> = 621). Hair (fur, whisker) samples were analyzed from specimens if no bone had been collected (<em>n</em> = 34). For some specimens (<em>n </em>= 18), both bone and fur were analyzed to determine the isotopic offset between these different tissues. We were unable to develop a protein purification method for skin samples to achieve reliable bulk isotope values, though skin values that yielded plausible C:N ratios are reported, some of which are for comparison to bone values (<em>n</em> = 17).</p>
<p>Hair samples, between 10 and 20 hairs with their follicles removed, were prepared for isotopic analysis by first washing with Milli-Q water. Then, lipids were removed via three rinses with petroleum ether in an ultrasonic bath (Thermo Fisher Scientific, Inc.) for 15 minutes each time, and other exogenous material was eliminated with alternating treatments of acid (0.5 M HCl) and base (0.1 M NaOH) until the solution was clear. After each acid or base treatment, five rinses with Milli-Q water were performed. Skin samples were treated similarly.</p>
<p><strong>Bulk stable isotope analysis:</strong><br />
For all bone and hair samples approximately 1 mg and 0.5 mg of sample, respectively, was weighed into tin cups (Costech, 3x5 mm) for elemental analysis-isotope ratio mass spectrometry (EA-IRMS). This analysis was performed at the Stable Isotope Lab (SIL) at the University of California (UC) Santa Cruz on a Carlo Erba EA 1108 elemental analyzer coupled to a Thermo-Finnigan Delta<sup>Plus</sup>&nbsp;XP isotope ratio mass spectrometer. δ<sup>15</sup>N values were referenced to an AIR standard, and δ<sup>13</sup>C values were referenced to a V-PDB standard. On a day-to-day basis, we measured and calibrated analyses with a laboratory IU Acetanilide standard (δ<sup>15</sup>N = 1.18‰, δ<sup>13</sup>C = -29.52‰, %N = 10.36%, %C = 71.02%) and a laboratory gelatin standard (δ<sup>15</sup>N = 5.60‰, δ<sup>13</sup>C = -12.60‰, %N = 16.44‰, %C = 44.02‰). The isotopic and concentration value of these laboratory standards are known by calibration to international standards (IAEA601, IAEA-346, USGS24, USGS25, USGS26, USGS34, USGS35, USGS41). We applied mass and drift corrections during each instrument session using the gelatin standard. Standard deviations for standards were &lt; 0.1 ‰ for both δ<sup>15</sup>N and δ<sup>13</sup>C and &lt;0.05 for C/N (seven PUGel standards analyzed at the start of each session and a PUGel and an Acetanilide standard analyzed after every eight samples during the session).</p>
<p><strong>Sample preparation for radiocarbon analysis:</strong><br />
When possible, skin samples from a specimen were analyzed for radiocarbon (<sup>14</sup>C), but when skin was unavailable, bone was analyzed instead. Prior to <sup>14</sup>C analysis, skin samples were manually cleaned to remove visible sand and dried in an oven. Bone samples required more extensive preparation to isolate collagen and eliminate contaminants.</p>
<p>Bone samples were prepared for <sup>14</sup>C according to an established laboratory protocol. First, between 150 and 200 mg of bone was weighed and ground into a coarse powder via a mortar and pestle (pre-cleaned with ethanol). Then, the material was transferred into a vial (BD Falcon 15 mL centrifuge tubes, polypropylene) for processing to isolate highly pure collagen. Ground bone was decalcified via the addition of 7 mL of HCl (0.5 M), agitation with a vortex, and storage at room temperature. Decalcifying samples were checked after 48 hours and if their decalcification was incomplete, the HCl was refreshed. Subsequently, the HCl was refreshed every 24 hours until decalcification appeared complete at which time the collagen was rinsed five times with Milli-Q water and 7 mL NaOH (0.1 M) was added at room temperature. After 24 hours, the NaOH was removed and the samples were rinsed five times with Milli-Q water. A final application of 7 mL of HCl (0.5 M) for 24 hours was performed to ensure complete decalcification, which was followed by five Milli-Q water rinses. Samples were kept frozen at -20 °C until the next preparatory step.</p>
<p>The bone collagen was gelatinized via the addition of 7 mL HCl (0.05 M) after being transferred to 10 mL borosilicate culture tubes (Fisherbrand). Samples were heated in the HCl solution at 58 °C on a hot plate for 48 hours. Immediately after stopping the gelatinization the samples were filtered (Whatman glass microfiber filters, grade 934-AH circles, particle retention 1.5 μm), retaining the filtrate, which was transferred to borosilicate culture tubes. Lastly, samples were dried via a vacuum concentrator centrifugal evaporator system (Jouan RC 10-10) with liquid N<sub>2</sub>&nbsp;and water traps. At this point, the nearly pure collagen from bone was obtained.</p>
<p><strong>Radiocarbon analysis:</strong><br />
After pretreatment, about 20 mg of each bone or skin sample was sent to the National Ocean Sciences Accelerator Mass Spectrometry Facility (NOSAMS) at Woods Hole Oceanographic Institution (WHOI) for <sup>14</sup>C analysis. Samples received further pretreatment to remove organic contaminants at NOASAMS (repeated acid-base rinse cycles until rinsing solutions were clear). NOSAMS used their organic combustion method to graphitize the samples, which were then pressed into target cartridge and loaded into the Accelerator Mass Spectrometer (AMS) for analysis. Samples were analyzed on either a 3 MV Tandetron or 500 kV Pelletron system. NBS Oxalic Acid I (NIST-SRM-4990) was the primary standard used for <sup>14</sup>C measurements, and process blank materials were analyzed during each instrument session. The blank materials were the Fourth International Radiocarbon Intercomparison (FIRI) A and B woods, as well as acetanilide (CE Elantech). More details on analyses at NOSAMS are available at: <a href="http://www.whoi.edu/nosams/home" target="_blank">http://www.whoi.edu/nosams/home</a></p>
<p>Upon receiving the data, <sup>14</sup>C ages were calibrated with CALIB 7.0.1, the Marine13 calibration database (Reimer et al. 2013), using the delta-<em>R</em> value of 791 +/- 121 (Hall et al. 2010). Calendar ages were reported as the midpoint of the one standard deviation range. The correction for the applied reservoir effect was verified via radiocarbon analysis of Weddell seal specimens from the Ross Sea that were of known age as they were collected during particular expeditions in the early 1900s. Additionally, an effect of contamination on the <sup>14</sup>C data was disregarded since preparation and analysis of standards resulted in <sup>14</sup>C measurements that had offsets from the known ages of the materials that were within instrument error. All all reported ages are relative to 1950. Not all samples could be calibrated and may immediately predate or postdate atmospheric nuclear testing. These samples have been assigned an age of 75.</p>
<p><strong>Sample preparation for ancient DNA analysis:</strong><br />
All ancient DNA (aDNA) work was conducted in a dedicated aDNA laboratory at Durham University, using strict protocols to prevent and detect contamination. Briefly, this included one-way movement of reagents, samples, and personnel from the aDNA to the modern DNA lab, decontamination using 50% bleach and/or UV sterilization, use of filter tips, and inclusion of extraction and negative controls every 10 to 20 samples.</p>
<p>Ancient DNA was extracted from skin, bone, and hair samples. For bone and skin samples, an ~ 1 cm x 1 cm section of sample was removed using a rotary saw with disposable blades. These were homogenized in a Retsch MM 200 mill in stainless steel canisters cleaned with Virkon disinfectant, 50% bleach, and rinsed in 95% ethanol. Hair samples were cut into ~ 5 mm portions using a sterile blade.</p>
<p><strong>aDNA extraction and amplification:</strong><br />
First, samples were digested overnight at 37 °C in 750 uL of solution of 0.5% SDS, 0.425 M EDTA (pH 8.0), 0.1 M Tris-HCl (pH 8.0), and 0.77 mg/mL Proteinase K. Following digestion, 3 mL of PB Buffer (QIAgen) was added to each sample, along with up to 50 uL of 3 M sodium acetate (pH 5.2) to adjust the pH for purification with the Qiaquick spin filter kit. Purification was conducted according to manufacturer directions; however, additional spins were required to bind the entire sample to the column. Elution was performed twice using 70 uL of EB buffer, which was incubated at 37 °C for 5 min.</p>
<p>Polymerase chain reaction (PCR) was carried out to amplify an approximately 180 bp fragment of the mitochondrial control region, using primers aSealCR1F (5’-GCATTAACGGTTTGCCCCAT-3’) and aSealCR1R (5’-GGTACACGTTTCACAAGGGT-3’), which were designed in the program Primer3 (Koressaar and Remm 2007, Untergasser et al. 2012) from 200 ancient southern elephant seal (sampled from the VLC; de Bruyn et al. 2009), 135 modern crabeater seal (Curtis et al. 2009), 83 modern Weddell seal (Curtis et al. 2009), and 2 modern leopard seal sequences from Genbank. This region carries several diagnostic sites that differ among the four species, thus facilitating species identification. PCR reactions were conducted in a total volume of 25 µl, which included 2 µl DNA, as well as 0.02 units of AmpliTaqGold, 1X AmpliTaq Gold buffer II, 2.5 mM MgCl<sub>2</sub>, 0.2 mM each dNTP, and 0.4 µM each primer. The thermocycler program used was 94 °C for 8 min, then 45 cycles of 94 °C for 30 s, 50 °C for 30 s, and 72 °C for 30 s, followed by a further extension step of 72 °C for 7 min. PCR products were visualized on a 2% agarose gel stained with ethidium bromide. In total, DNA extraction was attempted for 536 samples and was performed successfully for 468 samples.</p>
<p><strong>Species identification from aDNA analysis:</strong><br />
We developed a restriction digest test to conduct an initial screen for species identification. Positive PCR products (20 uL) were cleaned via a standard ethanol precipitation procedure: 10% of 3 M sodium acetate (pH 5.2) and 1 mL of chilled 100% ethanol was added to each sample, which was then incubated overnight at -20 °C. Samples were spun for 15 min and then the ethanol was discarded and 1 mL of chilled 70% ethanol was added. Samples were spun for another 15 min, the ethanol was discarded, and the samples were dried for 45 min at 50 °C in a SpeedVac DNA concentrator. Next, 15 uL of EB buffer, preheated to 55 °C, was added to each sample and the samples were subsequently incubated at 55 °C for a further 10 min in order for elution.</p>
<p>Restriction digests were carried out using 1x Cutsmart Buffer (New England Biolabs), 7.5 uL of cleaned PCR product, and 0.5 uL BstE-II HF enzyme (New England Biolabs). Reactions were incubated at 37 °C for 30 min and terminated by the addition of 5 uL of gel loading buffer, following manufacturer instructions. The resulting products were run at 90 V for 3 hr on a 2.5% agarose gel stained with ethidium bromide. <em>In silico</em> tests via the program, Geneious v9.0 (Kearse et al. 2012), suggested that this restriction digest would result in the production of two fragments of 100 and 80 bp in length for approximately 80% of the crabeater seal sequences available on Genbank. However, up to 2% of ancient southern elephant seals shared this site and would also be cut since no perfect species-specific restriction site could be found within the sequences available on Genbank (for this site or any other mitochondrial region) that would be short enough to reliably amplify aDNA. Any cut PCR product was assumed to be a crabeater seal, and any uncut product was sent for Sanger sequencing in the forward direction at Durham University’s DBS Genomics facility.</p>
<p>Resulting sequences were visually inspected and manually edited in Geneious and then compared against the Genbank database using the BLAST tool to provide initial species assignments. The highest scoring hit was accepted as long as the e-value was below 1 x 10<sup>-20</sup>&nbsp;and the sequence identity was greater than 95%. DNA sequences from Genbank, described above, were added to those obtained from our study. Sequences for northern elephant seal (<em>Mirounga angustirostris</em>), Mediterranean monk seal (<em>Monachus monachus</em>), Ross seal (<em>Ommatophoca rossii</em>), and bearded seal (<em>Erignathus barbatus</em>) were included as outgroups. MAFFT v7 (Katoh et al. 2002) was used to align the sequences and the best-fit model of nucleotide evolution was investigated using jModelTest v2 (Darriba et al. 2012). A neighbor-joining tree was built in Geneious with 1,000 bootstraps and principle component analysis (PCA) was conducted in the program GenAlEx (Peakall and Smouse 2006, 2012). Results (not shown) displayed all putative and known crabeater seal individuals grouping together in a monophyletic group with a bootstrap support of 89. Similarly, all northern and southern elephant seals grouped together with bootstrap support of 67, and Ross seals grouped together with support of 96. Leopard seals and Weddell seals grouped together in a single clade with a bootstrap support of 76, but these species are known to have a close evolutionary history (Dasmahapatra et al. 2009, Fulton and Strobeck 2010). PCA was able to successfully separate all species – both individuals of known identity and those with putative assignments – thus confirming previous initial BLAST species assignments. These species assignments have also been largely confirmed through morphological identification of preserved remains (e.g. teeth, body size). Additionally, eight individuals were tested two to three times with the restriction digest test and Sanger sequencing, and the results were consistent in each case.</p>
<p><strong>Cited references:</strong><br />
Ambrose SH (1990) Preparation and characterization of bone and tooth collagen for isotopic analysis. Journal of Archaeological Science 17:431-451. doi:<a href="http://dx.doi.org/10.1016/0305-4403(90)90007-R" target="_blank">10.1016/0305-4403(90)90007-R</a></p>
<p>Barwick RE, Balham RW (1967) Mummified Seal Carcases in a Deglaciated Region of South Victoria Land, Antarctica. Tuatara 15:165-180</p>
<p>Curtis C, Stewart BS, Karl SA (2009) Pleistocene population expansions of Antarctic seals. Molecular Ecology 18:2112-2121. doi:<a href="http://dx.doi.org/10.1111/j.1365-294X.2009.04166.x" target="_blank">10.1111/j.1365-294X.2009.04166.x</a></p>
<p>Darriba D, Taboada GL, Doallo R, Posada D (2012) jModelTest2: more models, new heuristics, and parallel computing. Nature Methods 9:772. doi:<a href="http://dx.doi.org/10.1038/nmeth.2109" target="_blank">10.1038/nmeth.2109</a></p>
<p>Dasmahapatra KK, Hoffman JI, Amos W (2009) Pinniped phylogenetic relationships inferred using AFLP markers. Heredity 103:168-177. doi:<a href="http://dx.doi.org/10.1038/hdy.2009.25" target="_blank">10.1038/hdy.2009.25</a></p>
<p>de Bruyn M, Hall BL, Chauke LF, Baroni C, Koch PL, Hoelzel AR (2009) Rapid response of a marine mammal species to Holocene climate and habitat change. PLoS Genetics 5:e1000554. doi:<a href="http://dx.doi.org/10.1371/journal.pgen.1000554" target="_blank">10.1371/journal.pgen.1000554</a></p>
<p>DeNiro MJ (1987) Stable isotopy and archaeology. American Scientist 75:182-191.&nbsp;<a href="http://www.jstor.org/stable/27854539" target="_blank">www.jstor.org/stable/27854539</a></p>
<p>Fulton TL and Strobeck C (2010) Multiple markers and multiple individuals refine true seal phylogeny and bring molecules and morphology back in line. Proceedings of the Royal Society B, Biological Sciences 277:1065-1070. doi:<a href="http://dx.doi.org/10.1098/rspb.2009.1783" target="_blank">10.1098/rspb.2009.1783</a></p>
<p>Hall BL, Henderson GM, Baroni C, Kellogg TB (2010) Constant Holocene Southern-Ocean <sup>14</sup>C reservoir ages and ice-shelf flow rates. Earth and Planetary Science Letters 296:115-123. doi:<a href="http://dx.doi.org/10.1016/j.epsl.2010.04.054" target="_blank">10.1016/j.epsl.2010.04.054</a></p>
<p>Katoh K, Misawa K, Kuma KI, Miyata T (2002) MAFFT: a novel method for rapid multiple sequence alignment based on fast Fourier transform. Nucleic Acids Research 29:4793-4799</p>
<p>Kearse M, Moir R, Wilson A, Stones-Havas S, Cheung M, Sturrock S, Buxton S, Cooper A, Markowitz S, Duran C, Thierer T, Ashton B, Mentjies P, Drummond A (2012) Geneious Basic: an integrated and extendable desktop software platform for the organization and analysis of sequence data. Bioinformatics 28:1647-1649. doi:<a href="http://dx.doi.org/10.1093/bioinformatics/bts199" target="_blank">10.1093/bioinformatics/bts199</a></p>
<p>Koressaar T, Remm M (2007) Enhancements and modifications of primer design program Primer3. Bioinformatics 23:1289-1291. doi:<a href="http://dx.doi.org/10.1093/bioinformatics/btm091" target="_blank">10.1093/bioinformatics/btm091</a></p>
<p>Peakall ROD and Smouse PE (2006) GENALEX 6: Genetic analysis in Excel. Population genetic software for teaching and research. Molecular Ecology Notes 6:288-295</p>
<p>Peakall ROD and Smouse PE (2012) GENALEX 6.5: Genetic analysis in Excel. Population genetic software for teaching and research, an update. Bioinformatics 28:2537-2539. doi:<a href="http://dx.doi.org/10.1093/bioinformatics/bts460" target="_blank">10.1093/bioinformatics/bts460</a></p>
<p>Reimer PJ, Bard E, Bayliss A, Beck JW, Blackwell PG, Ramsey CB, Buck CE, Cheng H, Edwards RL, Friedrich M, Grootes PM (2013). IntCal13 and Marine13 radiocarbon age calibration curves 0–50,000 years cal BP. Radiocarbon 55:1869-1887. doi:<a href="http://dx.doi.org/10.2458/azu_js_rc.55.16947" target="_blank">10.2458/azu_js_rc.55.16947</a></p>
<p>Todd LC (1987) Taphonomy of the Horner II Bone Bed. In The Horner Site, edited by GC Frison and LC Todd, pp. 107-198. Academic Press, Orlando.</p>
<p>Untergasser A, Cutcutache I, Koressaar T, Ye J, Faircloth BC, Remm M, Rozen SG (2012) Primer3--new capabilities and interfaces. Nucleic Acids Research 40:e115. doi:<a href="http://dx.doi.org/10.1093/nar/gks596" target="_blank">10.1093/nar/gks596</a></p>
Funding provided by NSF Office of Polar Programs (formerly NSF PLR) (NSF OPP) Award Number: OPP-1141849 Award URL: https://www.nsf.gov/awardsearch/show-award?AWD_ID=1141849
Funding provided by NSF Office of Polar Programs (formerly NSF PLR) (NSF OPP) Award Number: OPP-1142108 Award URL: https://www.nsf.gov/awardsearch/show-award?AWD_ID=1142108
completed
Brenda Hall
University of Maine
207-581-2191
School of Earth and Climate Sciences 5790 Bryand Global Sciences Center
Orono
ME
04469
US
brendah@maine.edu
pointOfContact
Paul L. Koch
University of California-Santa Cruz
831-234-9437
1156 High Street
Santa Cruz
CA
95064-1077
USA
plkoch@ucsc.edu
pointOfContact
Daniel P. Costa
University of California-Santa Cruz
831-459-2786
Dept. of Ecology and Evolutionary Biology, Ocean Health Building 100 Shaffer Road
Santa Cruz
CA
95060
USA
costa@ucsc.edu
pointOfContact
A. Rus Hoelzel
Durham University
44-0-191-3341325
Dept. of Biosciences, Durham University Stockton Road
Durham DH1 3LE
UK
a.r.hoelzel@durham.ac.uk
pointOfContact
asNeeded
Dataset Version: 1
Unknown
Sample_ID
Collection_date
General_area
Sampling_region
Latitude
Longitude
Altitude
Sample_types_collected
Brief_description
Age_class
Carcass_erosion_stage
Bone_weathering_stage
Taxon_field
Taxon_aDNA
Taxon_final
NOSAMS_lab_code
C14_age
C14_error
C14_d13C
Calendar_age
one_sigma
Sample_type_for_C14
C14_notes
d13C
d15N
C_to_N_atomic_ratio
Sample_type_for_isotopes
Accelerator Mass Spectrometer (AMS)
EA-IRMS
EA-IRMS
theme
None, User defined
sample identification
date
site description
latitude
longitude
No BCO-DMO term
sample type
comments
ageclass
sample description
taxon_code
carbon-14 age dating
d13C
d15N
Carbon to Nitrogen ratio (C:N)
featureType
BCO-DMO Standard Parameters
Accelerator Mass Spectrometer
Elemental Analyzer
Isotope-ratio Mass Spectrometer
Thermal Cycler
instrument
BCO-DMO Standard Instruments
otherRestrictions
otherRestrictions
Access Constraints: none. Use Constraints: Please follow guidelines at: http://www.bco-dmo.org/terms-use Distribution liability: Under no circumstances shall BCO-DMO be liable for any direct, incidental, special, consequential, indirect, or punitive damages that result from the use of, or the inability to use, the materials in this data submission. If you are dissatisfied with any materials in this data submission your sole and exclusive remedy is to discontinue use.
Collaborative Research: Exploring the Vulnerability of Southern Ocean Pinnipeds to Climate Change - An Integrated Approach
https://osprey.bco-dmo.org/project/726874
Collaborative Research: Exploring the Vulnerability of Southern Ocean Pinnipeds to Climate Change - An Integrated Approach
<p><em>NSF abstract:</em><br />
Building on previously funded NSF research, the use of paleobiological and paleogenetic data from mummified elephant seal carcasses found along the Dry Valleys and Victoria Land Coast in areas that today are too cold to support seal colonies (Mirougina leonina; southern elephant seals; SES) supports the former existence of these seals in this region. The occurrence and then subsequent disappearance of these SES colonies is consistent with major shifts in the Holocene climate to much colder conditions at the last ~1000 years BCE).</p>
<p>Further analysis of the preserved remains of three other abundant pinnipeds ? crabeater (Lobodon carciophagus), Weddell (Leptonychotes weddelli) and leopard (Hydrurga leptonyx) will be studied to track changes in their population size (revealed by DNA analysis) and their diet (studied via stable isotope analysis). Combined with known differences in life history, preferred ice habitat and ecosystem sensitivity among these species, this paleoclimate proxy data will be used to assess their exposure and sensitivity to climate change in the Ross Sea region during the past ~1-2,000 years</p>
Southern Ocean Pinnipeds
largerWorkCitation
project
eng; USA
biota
oceans
160.58937
164.72143
-78.9066
-76.67755
2013-01-16
2014-01-16
McMurdo Dry Valleys Region; Royal Society Range, Victoria Land Coast , Antarctic Peninsula, Amundsen Sea, Ross Sea
0
BCO-DMO catalogue of parameters from Location, weathering, bulk isotope, and 14C data for fossil seals from the western Ross Sea, Antarctica from from 2013-2014
Biological and Chemical Oceanography Data Management Office (BCO-DMO)
Unavailable
508-289-2009
WHOI MS#36
Woods Hole
MA
02543
USA
info@bco-dmo.org
http://www.bco-dmo.org
Monday - Friday 8:00am - 5:00pm
For questions regarding this resource, please contact BCO-DMO via the email address provided.
pointOfContact
http://lod.bco-dmo.org/id/dataset-parameter/732534.rdf
Name: Sample_ID
Units: unitless
Description: <p>Sample identification code</p>
http://lod.bco-dmo.org/id/dataset-parameter/732535.rdf
Name: Collection_date
Units: unitless
Description: <p>Date of sample collection formatted as yyyymmdd</p>
http://lod.bco-dmo.org/id/dataset-parameter/732536.rdf
Name: General_area
Units: unitless
Description: <p>General location of sampling</p>
http://lod.bco-dmo.org/id/dataset-parameter/732537.rdf
Name: Sampling_region
Units: unitless
Description: <p>More specific sampling location</p>
http://lod.bco-dmo.org/id/dataset-parameter/732538.rdf
Name: Latitude
Units: decimal degrees
Description: <p>Latitude of sample collection (negative values = south)</p>
http://lod.bco-dmo.org/id/dataset-parameter/732539.rdf
Name: Longitude
Units: decimal degrees
Description: <p>Longitude of sample collection (negative values = west; postivie values = east)</p>
http://lod.bco-dmo.org/id/dataset-parameter/732540.rdf
Name: Altitude
Units: meters above sea level (mas)
Description: <p>Altitude</p>
http://lod.bco-dmo.org/id/dataset-parameter/732541.rdf
Name: Sample_types_collected
Units: unitless
Description: <p>Type of tissues collected from specimen: B = bone, F = fur, N = nail, S = skin, T = tooth, W = whisker.</p>
http://lod.bco-dmo.org/id/dataset-parameter/732542.rdf
Name: Brief_description
Units: unitless
Description: <p>Narrative comments on the attributes of specimens</p>
http://lod.bco-dmo.org/id/dataset-parameter/732543.rdf
Name: Age_class
Units: unitless
Description: <p>Age class of specimen (adult, sub-adult, pup, unknown)</p>
http://lod.bco-dmo.org/id/dataset-parameter/732544.rdf
Name: Carcass_erosion_stage
Units: unitless
Description: <p>Measure of progressive carcass breakdown; Carcass Weathering Stage codes A-F modified from Barwick and Balham (1967). See Metadata Acquisition Description for definitions.</p>
http://lod.bco-dmo.org/id/dataset-parameter/732545.rdf
Name: Bone_weathering_stage
Units: unitless
Description: <p>Measure of progressive bone weathering and breakdown; Bone Weathering Stage codes 0-7 modified from Todd (1987). See Metadata Acquisition Description for definitions.</p>
http://lod.bco-dmo.org/id/dataset-parameter/732546.rdf
Name: Taxon_field
Units: unitless
Description: <p>Field identification of the specimen:Cr = crabeater seal,Lp = leopard seal,SES = southern elephant seal,Wd = Weddell seal,nd = not identifiable,? = tentative identification.</p>
http://lod.bco-dmo.org/id/dataset-parameter/732547.rdf
Name: Taxon_aDNA
Units: unitless
Description: <p>Identification through ancient DNA. See species codes above. Failed = aDNA attempt & failed; nd = aDNA not attempted.</p>
http://lod.bco-dmo.org/id/dataset-parameter/732548.rdf
Name: Taxon_final
Units: unitless
Description: <p>Final determination of species. See species codes above. U = unknown.</p>
http://lod.bco-dmo.org/id/dataset-parameter/732549.rdf
Name: NOSAMS_lab_code
Units: unitless
Description: <p>Identification code at the National Ocean Sciences Accelerator Mass Spectrometry facility</p>
http://lod.bco-dmo.org/id/dataset-parameter/732550.rdf
Name: C14_age
Units: years before present (1950)
Description: <p>Uncalibrated 14C age</p>
http://lod.bco-dmo.org/id/dataset-parameter/732551.rdf
Name: C14_error
Units: years
Description: <p>internal or external statistical error in 14C age (whichever is larger)</p>
http://lod.bco-dmo.org/id/dataset-parameter/732552.rdf
Name: C14_d13C
Units: permil (‰), V-PDB
Description: <p>?13C valued measured for 14C age estimate</p>
http://lod.bco-dmo.org/id/dataset-parameter/732553.rdf
Name: Calendar_age
Units: calendar years before present (1950)
Description: <p>Calendar years before present determined by 14C age. Samples that can't be calibrated set to 75 years.</p>
http://lod.bco-dmo.org/id/dataset-parameter/732554.rdf
Name: one_sigma
Units: years
Description: <p>1 sigma error on Calendar_age</p>
http://lod.bco-dmo.org/id/dataset-parameter/732555.rdf
Name: Sample_type_for_C14
Units: unitless
Description: <p>Type of sample used for 14C age determination:B = bone, F = fur, N = nail, S = skin, T = tooth, W = whisker.</p>
http://lod.bco-dmo.org/id/dataset-parameter/732556.rdf
Name: C14_notes
Units: unitless
Description: <p>Narrative comments on 14C</p>
http://lod.bco-dmo.org/id/dataset-parameter/732557.rdf
Name: d13C
Units: permil (‰), V-PDB
Description: <p>Stable carbon isotope value</p>
http://lod.bco-dmo.org/id/dataset-parameter/732558.rdf
Name: d15N
Units: permil (‰), AIR
Description: <p>Stable nitrogen isotope value</p>
http://lod.bco-dmo.org/id/dataset-parameter/732559.rdf
Name: C_to_N_atomic_ratio
Units: unitless
Description: <p>Atomic C to N ratio</p>
http://lod.bco-dmo.org/id/dataset-parameter/732560.rdf
Name: Sample_type_for_isotopes
Units: unitless
Description: <p>Type of sample used for isotopes:B = bone, F = fur, N = nail, S = skin, T = tooth, W = whisker.</p>
GB/NERC/BODC > British Oceanographic Data Centre, Natural Environment Research Council, United Kingdom
Biological and Chemical Oceanography Data Management Office (BCO-DMO)
Unavailable
508-289-2009
WHOI MS#36
Woods Hole
MA
02543
USA
info@bco-dmo.org
http://www.bco-dmo.org
Monday - Friday 8:00am - 5:00pm
For questions regarding this resource, please contact BCO-DMO via the email address provided.
pointOfContact
128053
https://darchive.mblwhoilibrary.org/bitstream/1912/29246/1/dataset-732524_fossil-seal-bulk-isotopes-14c__v1.tsv
download
https://doi.org/10.26008/1912/bco-dmo.732524.1
download
onLine
dataset
<p><strong>Sample collection:</strong><br />
Fossil seal samples were collected during the austral summers of 2005/06, 2006/07, 2012/13, and 2013/14 in Antarctica in the Dry Valleys and along the Victoria Land Coast (especially Inexpressible Island on Terra Nova Bay), Antarctica. Since this region experiences unusually dry and cold conditions, carcasses and bones are well-preserved, potentially for several thousand years, and therefore have unchanged isotopic compositions in most cases. The sampled species were crabeater, Weddell, leopard, and southern elephant seals. Latitude and longitude of each specimen was determined by GPS and recorded, and several photographs were taken of each specimen. Bone and carcass weathering states were determined. Several samples were gathered from the specimens. Most commonly, bone was collected, followed by skin and fur; nails, teeth, and whiskers were not frequently available for sampling, but taken when possible. Samples were collected with ethanol-cleaned tools, stored in Whirl-Pak bags, and refrigerated (~4 °C) when we returned from the field.</p>
<p><strong>Carcass and Bone Weathering:</strong><br />
For each specimen, we assessed the extent to which the carcass had been degraded by exposure, as well as the weathering state of exposed bone.</p>
<p>We assigned each specimen to one of the following Carcass Weathering Stages. These stages are modified from Barwick and Balham (1967):<br />
A&nbsp;= Complete.Fresh. Undamaged from wind erosion, no desiccation.<br />
B = Complete. Slightly weathered. Partial erosion of hair on exposed surfaces, cracks in skin exposing deeper tissues or bones in the flippers or cranium.<br />
C = Incomplete. Extensive erosion and exposure of bones of upward part of body (skull, ribs, limbs). Skeleton undamaged but soft tissues eroding between bony elements.<br />
D = Incomplete. Extensive erosion with regional destruction of bone and tissues. Vertebral column completely exposed and 40-50% tissue is destroyed.<br />
E = Very incomplete. &gt;50% of carcass is eroded. Vertebral column and cranium incomplete; limbs and rib cage becoming remnants. Difficult or impossible to identify species, sex, size.<br />
F = Fragments or isolated bones.</p>
<p>Bone Weathering Stages were determined on the most weathered bone from the carcass. Modified from Todd (1987).<br />
0 = unweathered and fatty.<br />
1 = unweathered, articular surfaces intact with no surface cracking.<br />
2 = articular surfaces intact with some surface cracking.<br />
3 = articular surfaces exhibit some deterioration, but &gt;50% of articular surface remains intact.<br />
4 = intact articular surface restricted to a few small "islands;" &lt;50% of articular surface remains intact.<br />
5 = no articular surface area remains intact.<br />
6 = bone severely deteriorated; large areas of fibrous bone exposed.<br />
7 = small weathered bone fragment or isolated tooth.</p>
<p><strong>Species identification:</strong><br />
When possible, species identification of each specimen was conducted in the field via examination of teeth or bones with features unique to the four pinniped species. Additionally, the team at the University of Durham in the United Kingdom extracted and analyzed DNA from many specimens, described below, to confirm or establish the species identification</p>
<p><strong>Sample preparation for bulk isotope analyses:</strong><br />
Preparation of bone samples was based on established procedures and by preliminary method testing in the lab (DeNiro 1987, Ambrose 1990). Bone fragments (50 -100 mg) were weighed into a vial (BD Falcon 15 mL centrifuge tubes, polypropylene) and acidified (to remove bone mineral, sedimentary carbonates, and fulvic acids) by the addition of 5 mL HCl (0.5 M) at room temperature. The acid was removed approximately three days later. If the samples did not appear completely decalcified (i.e., remains inflexible), a fresh aliquot of acid was added every 24 hours until the bone was decalcified, leaving behind bone collagen. Upon decalcification, the collagen was rinsed five times with Milli-Q water (Thermo Fisher Scientific, Inc.), neutralizing the sample, and 5 mL NaOH (0.1 M) was added to the samples, which were then kept at room temperature, further purifying the bone collagen by removing humic acids. A fresh aliquot of 0.1 M NaOH was added to the sample every 24 hours until the sample was nearly white. Again, the material was rinsed five times with Milli-Q water; then, it was refrigerated until the lipid extraction procedure. Lipids were removed via an accelerated solvent extraction with 100% petroleum ether (Dionex ASE 200 Accelerated Solvent Extractor: 1500 psi; 60°C; 3 cycles).</p>
<p>Bone was the most common sample type available. As it integrates diet over the largest period among the sample types collected (i.e., much of the animal’s lifespan), we analyzed bone from each specimen when available (<em>n</em> = 621). Hair (fur, whisker) samples were analyzed from specimens if no bone had been collected (<em>n</em> = 34). For some specimens (<em>n </em>= 18), both bone and fur were analyzed to determine the isotopic offset between these different tissues. We were unable to develop a protein purification method for skin samples to achieve reliable bulk isotope values, though skin values that yielded plausible C:N ratios are reported, some of which are for comparison to bone values (<em>n</em> = 17).</p>
<p>Hair samples, between 10 and 20 hairs with their follicles removed, were prepared for isotopic analysis by first washing with Milli-Q water. Then, lipids were removed via three rinses with petroleum ether in an ultrasonic bath (Thermo Fisher Scientific, Inc.) for 15 minutes each time, and other exogenous material was eliminated with alternating treatments of acid (0.5 M HCl) and base (0.1 M NaOH) until the solution was clear. After each acid or base treatment, five rinses with Milli-Q water were performed. Skin samples were treated similarly.</p>
<p><strong>Bulk stable isotope analysis:</strong><br />
For all bone and hair samples approximately 1 mg and 0.5 mg of sample, respectively, was weighed into tin cups (Costech, 3x5 mm) for elemental analysis-isotope ratio mass spectrometry (EA-IRMS). This analysis was performed at the Stable Isotope Lab (SIL) at the University of California (UC) Santa Cruz on a Carlo Erba EA 1108 elemental analyzer coupled to a Thermo-Finnigan Delta<sup>Plus</sup>&nbsp;XP isotope ratio mass spectrometer. δ<sup>15</sup>N values were referenced to an AIR standard, and δ<sup>13</sup>C values were referenced to a V-PDB standard. On a day-to-day basis, we measured and calibrated analyses with a laboratory IU Acetanilide standard (δ<sup>15</sup>N = 1.18‰, δ<sup>13</sup>C = -29.52‰, %N = 10.36%, %C = 71.02%) and a laboratory gelatin standard (δ<sup>15</sup>N = 5.60‰, δ<sup>13</sup>C = -12.60‰, %N = 16.44‰, %C = 44.02‰). The isotopic and concentration value of these laboratory standards are known by calibration to international standards (IAEA601, IAEA-346, USGS24, USGS25, USGS26, USGS34, USGS35, USGS41). We applied mass and drift corrections during each instrument session using the gelatin standard. Standard deviations for standards were &lt; 0.1 ‰ for both δ<sup>15</sup>N and δ<sup>13</sup>C and &lt;0.05 for C/N (seven PUGel standards analyzed at the start of each session and a PUGel and an Acetanilide standard analyzed after every eight samples during the session).</p>
<p><strong>Sample preparation for radiocarbon analysis:</strong><br />
When possible, skin samples from a specimen were analyzed for radiocarbon (<sup>14</sup>C), but when skin was unavailable, bone was analyzed instead. Prior to <sup>14</sup>C analysis, skin samples were manually cleaned to remove visible sand and dried in an oven. Bone samples required more extensive preparation to isolate collagen and eliminate contaminants.</p>
<p>Bone samples were prepared for <sup>14</sup>C according to an established laboratory protocol. First, between 150 and 200 mg of bone was weighed and ground into a coarse powder via a mortar and pestle (pre-cleaned with ethanol). Then, the material was transferred into a vial (BD Falcon 15 mL centrifuge tubes, polypropylene) for processing to isolate highly pure collagen. Ground bone was decalcified via the addition of 7 mL of HCl (0.5 M), agitation with a vortex, and storage at room temperature. Decalcifying samples were checked after 48 hours and if their decalcification was incomplete, the HCl was refreshed. Subsequently, the HCl was refreshed every 24 hours until decalcification appeared complete at which time the collagen was rinsed five times with Milli-Q water and 7 mL NaOH (0.1 M) was added at room temperature. After 24 hours, the NaOH was removed and the samples were rinsed five times with Milli-Q water. A final application of 7 mL of HCl (0.5 M) for 24 hours was performed to ensure complete decalcification, which was followed by five Milli-Q water rinses. Samples were kept frozen at -20 °C until the next preparatory step.</p>
<p>The bone collagen was gelatinized via the addition of 7 mL HCl (0.05 M) after being transferred to 10 mL borosilicate culture tubes (Fisherbrand). Samples were heated in the HCl solution at 58 °C on a hot plate for 48 hours. Immediately after stopping the gelatinization the samples were filtered (Whatman glass microfiber filters, grade 934-AH circles, particle retention 1.5 μm), retaining the filtrate, which was transferred to borosilicate culture tubes. Lastly, samples were dried via a vacuum concentrator centrifugal evaporator system (Jouan RC 10-10) with liquid N<sub>2</sub>&nbsp;and water traps. At this point, the nearly pure collagen from bone was obtained.</p>
<p><strong>Radiocarbon analysis:</strong><br />
After pretreatment, about 20 mg of each bone or skin sample was sent to the National Ocean Sciences Accelerator Mass Spectrometry Facility (NOSAMS) at Woods Hole Oceanographic Institution (WHOI) for <sup>14</sup>C analysis. Samples received further pretreatment to remove organic contaminants at NOASAMS (repeated acid-base rinse cycles until rinsing solutions were clear). NOSAMS used their organic combustion method to graphitize the samples, which were then pressed into target cartridge and loaded into the Accelerator Mass Spectrometer (AMS) for analysis. Samples were analyzed on either a 3 MV Tandetron or 500 kV Pelletron system. NBS Oxalic Acid I (NIST-SRM-4990) was the primary standard used for <sup>14</sup>C measurements, and process blank materials were analyzed during each instrument session. The blank materials were the Fourth International Radiocarbon Intercomparison (FIRI) A and B woods, as well as acetanilide (CE Elantech). More details on analyses at NOSAMS are available at: <a href="http://www.whoi.edu/nosams/home" target="_blank">http://www.whoi.edu/nosams/home</a></p>
<p>Upon receiving the data, <sup>14</sup>C ages were calibrated with CALIB 7.0.1, the Marine13 calibration database (Reimer et al. 2013), using the delta-<em>R</em> value of 791 +/- 121 (Hall et al. 2010). Calendar ages were reported as the midpoint of the one standard deviation range. The correction for the applied reservoir effect was verified via radiocarbon analysis of Weddell seal specimens from the Ross Sea that were of known age as they were collected during particular expeditions in the early 1900s. Additionally, an effect of contamination on the <sup>14</sup>C data was disregarded since preparation and analysis of standards resulted in <sup>14</sup>C measurements that had offsets from the known ages of the materials that were within instrument error. All all reported ages are relative to 1950. Not all samples could be calibrated and may immediately predate or postdate atmospheric nuclear testing. These samples have been assigned an age of 75.</p>
<p><strong>Sample preparation for ancient DNA analysis:</strong><br />
All ancient DNA (aDNA) work was conducted in a dedicated aDNA laboratory at Durham University, using strict protocols to prevent and detect contamination. Briefly, this included one-way movement of reagents, samples, and personnel from the aDNA to the modern DNA lab, decontamination using 50% bleach and/or UV sterilization, use of filter tips, and inclusion of extraction and negative controls every 10 to 20 samples.</p>
<p>Ancient DNA was extracted from skin, bone, and hair samples. For bone and skin samples, an ~ 1 cm x 1 cm section of sample was removed using a rotary saw with disposable blades. These were homogenized in a Retsch MM 200 mill in stainless steel canisters cleaned with Virkon disinfectant, 50% bleach, and rinsed in 95% ethanol. Hair samples were cut into ~ 5 mm portions using a sterile blade.</p>
<p><strong>aDNA extraction and amplification:</strong><br />
First, samples were digested overnight at 37 °C in 750 uL of solution of 0.5% SDS, 0.425 M EDTA (pH 8.0), 0.1 M Tris-HCl (pH 8.0), and 0.77 mg/mL Proteinase K. Following digestion, 3 mL of PB Buffer (QIAgen) was added to each sample, along with up to 50 uL of 3 M sodium acetate (pH 5.2) to adjust the pH for purification with the Qiaquick spin filter kit. Purification was conducted according to manufacturer directions; however, additional spins were required to bind the entire sample to the column. Elution was performed twice using 70 uL of EB buffer, which was incubated at 37 °C for 5 min.</p>
<p>Polymerase chain reaction (PCR) was carried out to amplify an approximately 180 bp fragment of the mitochondrial control region, using primers aSealCR1F (5’-GCATTAACGGTTTGCCCCAT-3’) and aSealCR1R (5’-GGTACACGTTTCACAAGGGT-3’), which were designed in the program Primer3 (Koressaar and Remm 2007, Untergasser et al. 2012) from 200 ancient southern elephant seal (sampled from the VLC; de Bruyn et al. 2009), 135 modern crabeater seal (Curtis et al. 2009), 83 modern Weddell seal (Curtis et al. 2009), and 2 modern leopard seal sequences from Genbank. This region carries several diagnostic sites that differ among the four species, thus facilitating species identification. PCR reactions were conducted in a total volume of 25 µl, which included 2 µl DNA, as well as 0.02 units of AmpliTaqGold, 1X AmpliTaq Gold buffer II, 2.5 mM MgCl<sub>2</sub>, 0.2 mM each dNTP, and 0.4 µM each primer. The thermocycler program used was 94 °C for 8 min, then 45 cycles of 94 °C for 30 s, 50 °C for 30 s, and 72 °C for 30 s, followed by a further extension step of 72 °C for 7 min. PCR products were visualized on a 2% agarose gel stained with ethidium bromide. In total, DNA extraction was attempted for 536 samples and was performed successfully for 468 samples.</p>
<p><strong>Species identification from aDNA analysis:</strong><br />
We developed a restriction digest test to conduct an initial screen for species identification. Positive PCR products (20 uL) were cleaned via a standard ethanol precipitation procedure: 10% of 3 M sodium acetate (pH 5.2) and 1 mL of chilled 100% ethanol was added to each sample, which was then incubated overnight at -20 °C. Samples were spun for 15 min and then the ethanol was discarded and 1 mL of chilled 70% ethanol was added. Samples were spun for another 15 min, the ethanol was discarded, and the samples were dried for 45 min at 50 °C in a SpeedVac DNA concentrator. Next, 15 uL of EB buffer, preheated to 55 °C, was added to each sample and the samples were subsequently incubated at 55 °C for a further 10 min in order for elution.</p>
<p>Restriction digests were carried out using 1x Cutsmart Buffer (New England Biolabs), 7.5 uL of cleaned PCR product, and 0.5 uL BstE-II HF enzyme (New England Biolabs). Reactions were incubated at 37 °C for 30 min and terminated by the addition of 5 uL of gel loading buffer, following manufacturer instructions. The resulting products were run at 90 V for 3 hr on a 2.5% agarose gel stained with ethidium bromide. <em>In silico</em> tests via the program, Geneious v9.0 (Kearse et al. 2012), suggested that this restriction digest would result in the production of two fragments of 100 and 80 bp in length for approximately 80% of the crabeater seal sequences available on Genbank. However, up to 2% of ancient southern elephant seals shared this site and would also be cut since no perfect species-specific restriction site could be found within the sequences available on Genbank (for this site or any other mitochondrial region) that would be short enough to reliably amplify aDNA. Any cut PCR product was assumed to be a crabeater seal, and any uncut product was sent for Sanger sequencing in the forward direction at Durham University’s DBS Genomics facility.</p>
<p>Resulting sequences were visually inspected and manually edited in Geneious and then compared against the Genbank database using the BLAST tool to provide initial species assignments. The highest scoring hit was accepted as long as the e-value was below 1 x 10<sup>-20</sup>&nbsp;and the sequence identity was greater than 95%. DNA sequences from Genbank, described above, were added to those obtained from our study. Sequences for northern elephant seal (<em>Mirounga angustirostris</em>), Mediterranean monk seal (<em>Monachus monachus</em>), Ross seal (<em>Ommatophoca rossii</em>), and bearded seal (<em>Erignathus barbatus</em>) were included as outgroups. MAFFT v7 (Katoh et al. 2002) was used to align the sequences and the best-fit model of nucleotide evolution was investigated using jModelTest v2 (Darriba et al. 2012). A neighbor-joining tree was built in Geneious with 1,000 bootstraps and principle component analysis (PCA) was conducted in the program GenAlEx (Peakall and Smouse 2006, 2012). Results (not shown) displayed all putative and known crabeater seal individuals grouping together in a monophyletic group with a bootstrap support of 89. Similarly, all northern and southern elephant seals grouped together with bootstrap support of 67, and Ross seals grouped together with support of 96. Leopard seals and Weddell seals grouped together in a single clade with a bootstrap support of 76, but these species are known to have a close evolutionary history (Dasmahapatra et al. 2009, Fulton and Strobeck 2010). PCA was able to successfully separate all species – both individuals of known identity and those with putative assignments – thus confirming previous initial BLAST species assignments. These species assignments have also been largely confirmed through morphological identification of preserved remains (e.g. teeth, body size). Additionally, eight individuals were tested two to three times with the restriction digest test and Sanger sequencing, and the results were consistent in each case.</p>
<p><strong>Cited references:</strong><br />
Ambrose SH (1990) Preparation and characterization of bone and tooth collagen for isotopic analysis. Journal of Archaeological Science 17:431-451. doi:<a href="http://dx.doi.org/10.1016/0305-4403(90)90007-R" target="_blank">10.1016/0305-4403(90)90007-R</a></p>
<p>Barwick RE, Balham RW (1967) Mummified Seal Carcases in a Deglaciated Region of South Victoria Land, Antarctica. Tuatara 15:165-180</p>
<p>Curtis C, Stewart BS, Karl SA (2009) Pleistocene population expansions of Antarctic seals. Molecular Ecology 18:2112-2121. doi:<a href="http://dx.doi.org/10.1111/j.1365-294X.2009.04166.x" target="_blank">10.1111/j.1365-294X.2009.04166.x</a></p>
<p>Darriba D, Taboada GL, Doallo R, Posada D (2012) jModelTest2: more models, new heuristics, and parallel computing. Nature Methods 9:772. doi:<a href="http://dx.doi.org/10.1038/nmeth.2109" target="_blank">10.1038/nmeth.2109</a></p>
<p>Dasmahapatra KK, Hoffman JI, Amos W (2009) Pinniped phylogenetic relationships inferred using AFLP markers. Heredity 103:168-177. doi:<a href="http://dx.doi.org/10.1038/hdy.2009.25" target="_blank">10.1038/hdy.2009.25</a></p>
<p>de Bruyn M, Hall BL, Chauke LF, Baroni C, Koch PL, Hoelzel AR (2009) Rapid response of a marine mammal species to Holocene climate and habitat change. PLoS Genetics 5:e1000554. doi:<a href="http://dx.doi.org/10.1371/journal.pgen.1000554" target="_blank">10.1371/journal.pgen.1000554</a></p>
<p>DeNiro MJ (1987) Stable isotopy and archaeology. American Scientist 75:182-191.&nbsp;<a href="http://www.jstor.org/stable/27854539" target="_blank">www.jstor.org/stable/27854539</a></p>
<p>Fulton TL and Strobeck C (2010) Multiple markers and multiple individuals refine true seal phylogeny and bring molecules and morphology back in line. Proceedings of the Royal Society B, Biological Sciences 277:1065-1070. doi:<a href="http://dx.doi.org/10.1098/rspb.2009.1783" target="_blank">10.1098/rspb.2009.1783</a></p>
<p>Hall BL, Henderson GM, Baroni C, Kellogg TB (2010) Constant Holocene Southern-Ocean <sup>14</sup>C reservoir ages and ice-shelf flow rates. Earth and Planetary Science Letters 296:115-123. doi:<a href="http://dx.doi.org/10.1016/j.epsl.2010.04.054" target="_blank">10.1016/j.epsl.2010.04.054</a></p>
<p>Katoh K, Misawa K, Kuma KI, Miyata T (2002) MAFFT: a novel method for rapid multiple sequence alignment based on fast Fourier transform. Nucleic Acids Research 29:4793-4799</p>
<p>Kearse M, Moir R, Wilson A, Stones-Havas S, Cheung M, Sturrock S, Buxton S, Cooper A, Markowitz S, Duran C, Thierer T, Ashton B, Mentjies P, Drummond A (2012) Geneious Basic: an integrated and extendable desktop software platform for the organization and analysis of sequence data. Bioinformatics 28:1647-1649. doi:<a href="http://dx.doi.org/10.1093/bioinformatics/bts199" target="_blank">10.1093/bioinformatics/bts199</a></p>
<p>Koressaar T, Remm M (2007) Enhancements and modifications of primer design program Primer3. Bioinformatics 23:1289-1291. doi:<a href="http://dx.doi.org/10.1093/bioinformatics/btm091" target="_blank">10.1093/bioinformatics/btm091</a></p>
<p>Peakall ROD and Smouse PE (2006) GENALEX 6: Genetic analysis in Excel. Population genetic software for teaching and research. Molecular Ecology Notes 6:288-295</p>
<p>Peakall ROD and Smouse PE (2012) GENALEX 6.5: Genetic analysis in Excel. Population genetic software for teaching and research, an update. Bioinformatics 28:2537-2539. doi:<a href="http://dx.doi.org/10.1093/bioinformatics/bts460" target="_blank">10.1093/bioinformatics/bts460</a></p>
<p>Reimer PJ, Bard E, Bayliss A, Beck JW, Blackwell PG, Ramsey CB, Buck CE, Cheng H, Edwards RL, Friedrich M, Grootes PM (2013). IntCal13 and Marine13 radiocarbon age calibration curves 0–50,000 years cal BP. Radiocarbon 55:1869-1887. doi:<a href="http://dx.doi.org/10.2458/azu_js_rc.55.16947" target="_blank">10.2458/azu_js_rc.55.16947</a></p>
<p>Todd LC (1987) Taphonomy of the Horner II Bone Bed. In The Horner Site, edited by GC Frison and LC Todd, pp. 107-198. Academic Press, Orlando.</p>
<p>Untergasser A, Cutcutache I, Koressaar T, Ye J, Faircloth BC, Remm M, Rozen SG (2012) Primer3--new capabilities and interfaces. Nucleic Acids Research 40:e115. doi:<a href="http://dx.doi.org/10.1093/nar/gks596" target="_blank">10.1093/nar/gks596</a></p>
Specified by the Principal Investigator(s)
<p><strong>BCO-DMO Processing:</strong><br />
-modified parameter names (replaced spaces with underscores);<br />
-changed date format from mm/dd/yyyy to yyyymmdd;<br />
-there were two dates with a year of 3013; changed to 2013 (Samples "HGB-12-51,52,53 (ECB-12-01,-02,-03)" and "HGB-12-52").</p>
Specified by the Principal Investigator(s)
asNeeded
7.x-1.1
Biological and Chemical Oceanography Data Management Office (BCO-DMO)
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info@bco-dmo.org
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For questions regarding this resource, please contact BCO-DMO via the email address provided.
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Accelerator Mass Spectrometer (AMS)
Accelerator Mass Spectrometer (AMS)
PI Supplied Instrument Name: Accelerator Mass Spectrometer (AMS) PI Supplied Instrument Description:NOSAMS used their organic combustion method to graphitize the samples, which were then pressed into target cartridge and loaded into the Accelerator Mass Spectrometer (AMS) for analysis. Instrument Name: Accelerator Mass Spectrometer Instrument Short Name:AMS Instrument Description: An AMS measures "long-lived radionuclides that occur naturally in our environment. AMS uses a particle accelerator in conjunction with ion sources, large magnets, and detectors to separate out interferences and count single atoms in the presence of 1x1015 (a thousand million million) stable atoms, measuring the mass-to-charge ratio of the products of sample molecule disassociation, atom ionization and ion acceleration." AMS permits ultra low-level measurement of compound concentrations and isotope ratios that traditional alpha-spectrometry cannot provide. More from Purdue University: http://www.physics.purdue.edu/primelab/introduction/ams.html Community Standard Description: http://vocab.nerc.ac.uk/collection/L05/current/LAB17/
EA-IRMS
EA-IRMS
PI Supplied Instrument Name: EA-IRMS PI Supplied Instrument Description:This analysis was performed at the Stable Isotope Lab (SIL) at the University of California (UC) Santa Cruz on a Carlo Erba EA 1108 elemental analyzer coupled to a Thermo-Finnigan DeltaPlus XP isotope ratio mass spectrometer. Instrument Name: Elemental Analyzer Instrument Short Name: Instrument Description: Instruments that quantify carbon, nitrogen and sometimes other elements by combusting the sample at very high temperature and assaying the resulting gaseous oxides. Usually used for samples including organic material. Community Standard Description: http://vocab.nerc.ac.uk/collection/L05/current/LAB01/
EA-IRMS
EA-IRMS
PI Supplied Instrument Name: EA-IRMS PI Supplied Instrument Description:This analysis was performed at the Stable Isotope Lab (SIL) at the University of California (UC) Santa Cruz on a Carlo Erba EA 1108 elemental analyzer coupled to a Thermo-Finnigan DeltaPlus XP isotope ratio mass spectrometer. Instrument Name: Isotope-ratio Mass Spectrometer Instrument Short Name:IR Mass Spec; IRMS Instrument Description: The Isotope-ratio Mass Spectrometer is a particular type of mass spectrometer used to measure the relative abundance of isotopes in a given sample (e.g. VG Prism II Isotope Ratio Mass-Spectrometer). Community Standard Description: http://vocab.nerc.ac.uk/collection/L05/current/LAB16/
PI Supplied Instrument Name: Instrument Name: Thermal Cycler Instrument Short Name:Thermal Cycler Instrument Description: A thermal cycler or "thermocycler" is a general term for a type of laboratory apparatus, commonly used for performing polymerase chain reaction (PCR), that is capable of repeatedly altering and maintaining specific temperatures for defined periods of time. The device has a thermal block with holes where tubes with the PCR reaction mixtures can be inserted. The cycler then raises and lowers the temperature of the block in discrete, pre-programmed steps. They can also be used to facilitate other temperature-sensitive reactions, including restriction enzyme digestion or rapid diagnostics.
(adapted from http://serc.carleton.edu/microbelife/research_methods/genomics/pcr.html)