MARINE MAMMAL SCIENCE, 25(1): 229–238 ( January 2009) C 2008 by the Society for Marine Mammalogy DOI: 10.1111/j.1748-7692.2008.00248.x Molecular species identification of historical whale remains from South Georgia CHARLOTTE LINDQVIST ANJA PROBST Natural History Museum, University of Oslo, P. O. Box 1172, Blindern, N-0318 Oslo, Norway E-mail: charlotte.lindqvist@nhm.uio.no ANTHONY R. MARTIN British Antarctic Survey, High Cross, Madingley Road, Cambridge CB3 OET, United Kingdom ØYSTEIN WIIG LUTZ BACHMANN Natural History Museum, University of Oslo, P. O. Box 1172, Blindern, N-0318 Oslo, Norway The island of South Georgia is located at the southern extreme of the South Atlantic Ocean, on the edge of the Southern Ocean that surrounds Antarctica. Intensive commercial whaling at South Georgia began in 1904, when the first land-based whaling station was built in Grytviken (54◦ 17 S, 36◦ 30 W). Five other shore stations were eventually built: Ocean Harbour (54◦ 20 S, 36◦ 16 W), Leith Harbour (54◦ 08 S, 36◦ 41 W), Husvik Harbour (54◦ 18 S, 36◦ 71 W), Stromness Harbour (54◦ 90 S, 36◦ 41 W), and Prince Olav Harbour (54◦ 40 S, 36◦ 90 W). Another site, Godthul (54◦ 17 S, 36◦ 17 W), was used as a protected anchorage for floating factories. By 1965, when shore-based whaling activity ceased, over 175,000 whales had been processed on the island (Moore et al. 1999). The once abundant stocks of baleen whales in the Antarctic had at that time been reduced to about a third of their former sizes (Laws 1977). When considering blue (Balaenoptera musculus), fin (B. physalus), sei (B. borealis), and humpback (Megaptera novaeangliae) whales together, the average population size was reduced to ca. 18% (Laws 1977). Humpback and blue whales experienced the most severe bottlenecks, having been reduced to about 3% and 5% of the estimated initial populations, respectively. According to more recent estimates, even 80%–95% of the pristine populations of humpback, blue, and fin whales have been killed (Baker and Clapham 2002). For the blue whales depletion to even less than 1% of the pre-exploitation population size has been reported (Branch et al. 2004, 2007). Currently, knowledge about the recovery from the bottlenecks and current population sizes, structures, and migration patterns are important issues 229 230 MARINE MAMMAL SCIENCE, VOL. 25, NO. 1, 2009 in the conservation of Southern Hemisphere baleen whales. In this context, insight into historical population structures would be of great value. The processing of thousands of whales rendered an enormous number of bone remains that were dumped in the vicinity of the whaling stations on South Georgia or in the sea. Today, these bones may be a unique source for retrieving genetic information that would aid the study of the genetic structure of historical whale populations prior to human exploitation. Examining the genetic variation of preand postwhaling populations of different Southern Hemisphere whale species could offer an opportunity to elucidate the differences in their respective exploitation histories as well as the effects of migration patterns and postwhaling recovery on the levels and distribution of genetic variation. Extraction of nucleic acids from historical samples has become relatively commonplace, and a number of recent studies have applied the ancient DNA methodology for the genetic analyses of historical whale remains (e.g., Rosenbaum et al. 1997; Pichler et al. 2001; Dalebout et al. 2003, 2004; Rastogi et al. 2004; Borge et al. 2007). However, the success rates remain unpredictable depending on the particular environmental conditions to which a sample was exposed. Since DNA and organic molecules are expected to survive longer in colder environments (Willerslev et al. 2004), the constant low temperatures on and around South Georgia may have been more favorable for DNA survival (Smith et al. 2001, Lambert et al. 2002) than is the case for, e.g., museum specimens. Maternally inherited mitochondrial DNA (mtDNA) has been the most frequently applied genetic marker in phylogenetic and population genetic studies of historical animal samples. It has been argued that its relatively high copy number increases the likelihood for extracting suitable template DNA (Handt et al. 1994). Moreover, due to the continuous increase of DNA sequence data and widespread and continuing use of mtDNA sequence data in cetacean studies as well, particularly of mitochondrial cytochrome oxidase I (cox I), cytochrome b (cyt b), and control region (CR) sequences as well as complete mtDNA genomes, mtDNA markers are highly suited for molecular diagnostics studies. In the current study we present a proof-of-concept approach to molecular identification of historical whale remains from South Georgian whaling stations. We attempted to extract DNA from 44 whalebones and dried muscle samples collected at four localities on South Georgia (Table 1). Bone samples were all collected from shore sites, and most have been exposed to sunlight, although over the years some samples may have been buried temporarily under stones or other bones. Air-dried meat samples were collected from a single drying frame. During the experiments, all background information on the samples was kept blind to the experimenters. Because the bone samples were collected randomly from beaches around several whaling stations, and bones must have been mixed up after up to 100 years of ice, wind, and waves moving them around on the boulder pavements it seems very unlikely that different bone fragments belong to the same individual. However, in the case of the dried muscle tissue it is possible that the multiple samples were derived from the same individual. In any case, redundant sampling does not pose a problem in the current study because the aim was molecular species identification not genetic Sample ID G1 G2 G3 G4 G5 G6 G7 G8 G9 G10 G11 G12 G13 G14 G15 G16 G17 G18 G19 G20 G21 L1 L2 L3 L4 L5 Type of materiala DB DB DB DB DB DB DB DB DB DB DB DB DB DB DB DB MDB DB MDB DB MDB MDB MDB DB DB DB A x x x x x x – x x – x x x x x – x x x x x x x – – – B x x x x x x – – – – – – – – – – x x x x x – x – – – Amplificationb Haplotypec G1 G1 G3 G4 G1 G6 – G8A G8A – G8A G8A G13A G8A G8A – G4 G1 G1 G1 G1 L1A L2 – – – Species annotationd MP-analysis Humpback Humpback Fin Humpback Humpback Humpback – Humpback Humpback – Humpback Humpback Fin Humpback Humpback – Humpback Humpback Humpback Humpback Humpback Sei Fin – – – Table 1. Samples used in the present study and positive species identifications. NOTES 231 GenBank accession no. EU831245 EU831246 EU831262 EU831243 EU831247 EU831242 – EU831248 EU831249 – EU831250 EU831251 EU831263 EU831252 EU831253 – EU831244 EU831254 EU831255 EU831256 EU831257 EU831266 EU831264 – – – (Continued) Type of materiala MDB MDB DB MDB M M M M M M M DB DB DB DB MDB MDB MDB A – – – x x x x x x – x x – x x x – x B – – – – – – – x x – – x – – – – – – Amplificationb Haplotypec – – – L9A L9A L9A L9A M4 M4 – L9A G1 – G8A G13A G8A – G8A Species annotationd MP-analysis – – – Sei Sei Sei Sei Sei Sei – Sei Humpback – Humpback Fin Humpback – Humpback GenBank accession no. – – – EU831267 EU831268 EU831269 EU831270 EU831271 EU831272 – EU831273 EU831258 – EU831259 EU831265 EU831260 – EU831261 a DB, dense bones such as bullae and similar material from the head; MDB, medium dense bones such as the outermost part of long bones; M, air dried meat. b Fragment A was amplified with the “A2dir” and “A1rev” primers, and fragment B with the “B1dir” and “B1rev” primers (see Table 2). c Assigned only for the purpose of this study. d “Witness for the Whales” web identification tool (http://www.cebl.auckland.ac.nz:9000/page/whales/title; Ross et al. 2003) assigned the submitted sequences to the very same species as the presented maximum parsimony analysis. Sample ID L6 L7 L8 L9 M1 M2 M3 M4 M5 M6 M7 OH1 OH2 OH3 U1 U2 U3 U4 Table 1 (Continued) 232 MARINE MAMMAL SCIENCE, VOL. 25, NO. 1, 2009 NOTES 233 differentiation of individuals or population genetic estimates such as, e.g., nucleotide or haplotype diversity. For the purpose of rapidly identifying any historical baleen whale sample with reasonable confidence, we designed a robust assay that targets two short stretches (180 base pairs and 131 base pairs) of the mitochondrial cyt b gene. Successful PCR amplification and subsequent sequencing of the PCR products are in most instances expected to permit species determination from samples with reasonable DNA preservation. Previous studies have shown that short fragments of the cyt b gene have a very high taxonomic power for identification to species of whale samples (Dalebout et al. 2004 and references therein). The proper initial species identification of historical bone samples is particularly important for selecting appropriate primers for downstream population-level analyses that target more variable genetic markers such as, e.g., microsatellite loci and/or the mitochondrial CR. In such downstream analyses, more variable markers may be used to determine genetic diversity and haplotype frequencies of modern vs. historical populations. Furthermore, such data may also provide estimates of the historical population size (Roman and Palumbi 2003, Alter et al. 2007). When working with historical samples, stringent DNA protocols are particularly important (Cooper and Poinar 2000). Due to the small amounts and degraded nature of recovered ancient DNA, controls for contamination require particular attention. Contamination can occur at any stage in the processing of ancient bone DNA, but it is particularly prevalent during sample preparation when the bone material is ground into a powder fine enough for the extraction of DNA. In this study, chopping and grinding of bone material was conducted in a different building physically isolated from the DNA facility. Furthermore, in the DNA laboratory, no analyses of any modern whale material of the species in question had ever taken place. All DNA extractions and PCR reactions were set up in hoods equipped with UV-light in a facility well separated from the labs where subsequent purifications and sequencing of the PCR products were performed. Small samples of bone material were chopped off with a hammer and chisel. The bone fragments and the dried muscle samples were then ground into fine powder in a mortar under liquid nitrogen. Mortars and pestles were cleaned with 5% deconex, rinsed with distilled water and 70% EtOH, wrapped in aluminum foil and baked at ca. 120◦ C overnight in order to avoid carry-over contamination between samples. Approximately 0.1 g of bone powder was subsequently transferred into 2.0 mL screwcapped centrifuge tubes, and DNA was extracted according to Borge et al. (2007). DNA sequences of the cyt b gene were aligned for several cetacean species retrieved from the NCBI database in order to identify conserved areas. Based on sequences from fin whale (GenBank acc. no. X61145; Arnason et al. 1991) and sei whale (GenBank acc. no. X75582; Arnason and Gullberg 1994) primers were designed in conserved areas in the 5 -end of the cyt b gene using the free online software Primer3 (Rozen and Skaletsky 2000). Because DNA from historical samples can be highly degraded it is necessary to design primers to amplify relatively shorter fragments than otherwise is the case. Two sets of primers were designed (Table 2): the primers “A2dir” and “A1rev” amplified a fragment A of 180 base pairs (bp), whereas the “B1dir” and 234 MARINE MAMMAL SCIENCE, VOL. 25, NO. 1, 2009 Table 2. Cytochrome b primers designed and used for species identification. Amplicon Primer Positiona Sequence (5 –3 ) A A2dir A1rev B1dir B1rev 3–25 161–182 161–182 270–291 GACCAACATCCGAAAAACACACC GTTGTTGTGTCTGGTGTGTAGT ACTACACACCAGACACAACAAC GTGGGCGTAGAGGCAGATGAAG B a Nucleotide positions correspond to the complete cytochrome b sequence from Balaenoptera physalus (X61145) and B. borealis (X75582). Figure 1. Phylogenetic analysis of 28 cytochrome b sequences, including 10 partial sequences determined for historical bone samples from South Georgia (marked in bold). Strict consensus tree of three most-parsimonious trees with bootstrap values above 50% shown below branches. GenBank accession numbers are shown in parenthesis after taxon name of the sequences retrieved from the NCBI database. “B1rev” primers amplified an adjacent fragment B of 131 bp, providing a total of 289 bp when both fragments were amplified and sequenced. Primers A1rev and B1dir are reverse complements of each other and the contiguous 289 bp consisting of fragments A and B are therefore invariant for 67 bp, i.e., 222 bp can be informative for species identification, 135 bp for fragment A and 87 bp for fragment B. As expected (Dalebout et al. 2004) and illustrated in Figure 1, the targeted 222 bp of the cyt b gene NOTES 235 provide already a high diagnostic power for species identification. PCR amplifications were performed in 25 L reaction volumes using 1U PfuTurbo DNA polymerase in 1× Reaction Buffer (Stratagene, La Jolla, CA, USA), 0.2 mmol/L of each dNTP, 0.04% bovine serum albumen (BSA), 1 mol/L of each primer, and 2 L of unquantified genomic template DNA. Thermal cycling conditions were optimized using different annealing temperatures in the range 48◦ –58◦ C and the following protocol yielded the highest number of successful amplifications for both fragments: 94◦ C for 2 min; 35 cycles of 94◦ C for 50 s, 54◦ C for 50 s, and 72◦ C for 1 min; and a final extension at 72◦ C for 10 min. PCR products were purified by incubation at 37◦ C for 30 min with 8 L of 1:10 strength diluted exoSAP-IT (USB Corporation, Cleveland, OH, USA) per reaction. Cycle sequencing of the purified PCR products, using the same primers as in the PCR reaction, was performed in 10 L reactions using 1 L BigDye Terminator Cycle Sequencing Ready Reaction Kit V 1.1 (Applied Biosystems), 3 L 5× Sequencing Buffer, 10 pmol primer, and 3 L cleaned PCR product. Sequencing products were purified with ethanol precipitation and analyzed using an ABI 3100 Genetic Analyzer (Applied Biosystems, Foster City, CA, USA). Forward and reverse sequences were assembled and edited using Sequencher version 4.1.4 (GeneCodes, Ann Arbor, MI, USA). Of the 44 samples, 32 samples (72.7%) were successfully amplified and sequenced for fragment A. There was no difference in the success rate depending on the type of material (see Table 1). Of these, 15 samples (34.1%) also gave positive amplification and sequences for fragment B (Table 1). Thus, the primer pair targeting fragment A (180 bp) was more suitable for degraded DNA templates than that targeting fragment B (131 bp), which is in line with the results of the Primer3 (Rozen and Skaletsky 2000) search for suitable primer pairs. BLAST sequence similarity searches (Altschul et al. 1990, Zhang et al. 2000) of the retrieved sequences against the nonredundant (nr) NCBI database (http://www.ncbi.nlm.nih.gov) using the default settings confirmed that all sequences represented baleen whales. In order to determine the species identity of the South Georgia whale remains, a large number of cyt b sequences of cetaceans representing a broad taxonomic range of taxa within the order were retrieved from the NCBI database, including all baleen whale species found in Antarctic waters. These baleen reference sequences, two odontocete sequences, Orcinus orca and Physeter macrocephalus, which are also found in Antarctic water, and haplotypes for the sequences generated in this study (see Table 1) were unambiguously aligned manually using the software package BioEdit (Hall 1999). The two odontocete sequences were used as the outgroup. The data matrix consisting of a total of 28 sequences (18 from GenBank and 10 haplotypes determined in this study) was subjected to parsimony analyses using the program TNT (Goloboff et al. 2003) and the traditional search option with default settings (Wagner tree with 100 random replications and saving 10 trees per replication). Additional tree bisection reconnection (TBR) branch swapping was performed on trees resulting from the initial search to find additional equally parsimonious trees. A strict consensus tree was calculated from the three most-parsimonious trees found. To estimate support for internal branches, parsimony bootstrapping was performed in TNT, using 1000 bootstrap replicates, 236 MARINE MAMMAL SCIENCE, VOL. 25, NO. 1, 2009 each performing TBR branch swapping with 10 random entry orders and saving 1 tree per replicate. The 32 historical samples were all successfully identified taxonomically with reasonable confidence (bootstrap support > 80, following, e.g., Dalebout et al. 2004). The samples were identified as derived from fin whales, humpback whales, or from a member of the sei whale/Bryde’s whale (Balaenoptera brydei)/pygmy Bryde’s whale (B. edeni) clade (Fig. 1, Table 1). No blue whale samples were detected, which is not surprising since blue whales were mostly hunted after the stations were forced to process the whole carcass, including use of the bones for extraction of oil, hence leaving no bones at the site. The majority of the samples (four haplotypes) were classified as humpback whales. Four samples (three haplotypes) were identified as fin whales, and the remaining eight samples (three haplotypes) grouped in a strongly supported clade including two reference sequences from sei whales as well as one each from Brydes and pygmy Bryde’s whale. Trimming the sequences retrieved from GenBank to the same length as the query sequences (i.e., 180 bp) yielded the same species identification for the unknown samples. Recent genetic studies have indicated some taxonomic uncertainties relating to the sei, Bryde’s, and pygmy Bryde’s whale species complex (Wada and Numachi 1991, Yoshida and Kato 1999). Combining SINE insertion and mitochondrial sequence data led Sasaki et al. (2005, 2006) and Nikaido et al. (2006) to conclude that Bryde’s and pygmy Bryde’s whales constitute a sister taxon to sei whale. Because Bryde’s and pygmy Bryde’s whales have not been reported in Antarctic waters, the eight included samples L1, L9, M1–5 and M7 were considered as representing sei whale. To further test the validity of the approach presented here, the obtained cyt b sequences were submitted to the web-based species identification tool “Witness for the Whales” (http://www.cebl.auckland.ac.nz:9000/page/whales/title). The tool offers species identification for submitted nucleotide sequences of the mitochondrial cyt b and CR through maximum likelihood analysis (Ross et al. 2003) using a purpose-compiled, specialist-curated database that includes multiple representatives for the majority of recognized cetacean species. Using both the simple and advanced search modes, the web tool assigned the submitted sequences to the very same species as in the maximum parsimony analysis presented here (Table 1). To summarize, in the present study we demonstrated that sufficient native DNA suitable for PCR amplifications of short mtDNA fragments (at least 180 bp) can be extracted from a large number of historical whale samples from South Georgia. Amplification and sequencing of two stretches of the mitochondrial cyt b gene offers an easy and rapid approach to identifying samples suitable for further genetic analyses and to determine the species status of whale remains with reasonable confidence. At least for humpback, fin, and sei whales, South Georgia provides suitable material for studying historical population structures. ACKNOWLEDGMENTS We are grateful for funding from the Natural History Museum, University of Oslo and the British Antarctic Survey. We thank Victor A. Albert for helpful comments. 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