Native to southern Africa, the blue antelope (Hippotragus leucophaeus) is the only large African mammal species known to have become extinct in historical times. However, it was poorly documented prior to its extinction ~ 1800 AD, and many of the small number of museum specimens attributed to it are taxonomically contentious. This places limitations on our understanding of its morphology, ecology, and the mechanisms responsible for its demise. We retrieved genetic information from ten of the sixteen putative blue antelope museum specimens using both shotgun sequencing and mitochondrial genome target capture in an attempt to resolve the uncertainty surrounding the identification of these specimens. We found that only four of the ten investigated specimens, and not a single skull, represent the blue antelope. This indicates that the true number of historical museum specimens of the blue antelope is even smaller than previously thought, and therefore hardly any reference material is available for morphometric, comparative and genetic studies. Our study highlights how genetics can be used to identify rare species in natural history collections where other methods may fail or when records are scarce. Additionally, we present an improved mitochondrial reference genome for the blue antelope as well as one complete and two partial mitochondrial genomes. A first analysis of these mitochondrial genomes indicates low levels of maternal genetic diversity in the ‘museum population’, possibly confirming previous results that blue antelope population size was already low at the time of the European colonization of South Africa.
The blue antelope, Hippotragus leucophaeus (Pallas, 1766), is the first and only large African mammal species to become extinct in historical times1,2 (Fig. 1a). Endemic to southern Africa, during the seventeenth and eighteenth century, the blue antelope (also called bluebuck, blaauwbok or bloubok) was confined to a very limited range between Caledon, Swellendam and Bredasdorp3,4 (Fig. 1b). However, the Pleistocene and Holocene fossil record documents its presence across a much larger, albeit still relatively restricted, area along the coastal plains of the Cape Floristic Region5,6,7 and possibly also in the highlands of Lesotho8. Its name derives from its pelt color, which was perceived to be bluish-grey while the animal was alive, with a distinctive white patch in front of the eye (leucophaeus is Greek for ‘white–grey’)9,10 (Fig. 1a).
The blue antelope was likely first mentioned in writing by J. Schreyer in 16794,11. P. Kolb12 was the first to characterize it in more detail when he encountered it during his travels near Caledon in 1708. It was first formally described as Antilope leucophaea in 1766 by P. S. Pallas, based on several skins in The Hague9. Around 1800, only about 100 years after it was first mentioned, the blue antelope went extinct13,14.
Its extinction has generally been attributed to competition with and habitat deterioration by livestock5,15, disruption of migratory pathways both in prehistoric times and through Colonial-era habitat transformation6, and overhunting by European colonists1,2. Using a modelling approach, Kerley et al.16 found that its population size was already small (about 370 individuals) with a small distribution range, and that the species therefore was highly vulnerable at the time of European colonization (mid-seventeenth century). These authors concluded that hunting by European colonists drove the blue antelope to extinction, but that it was not the only force leading to its demise. The growing demand of European collectors to own a specimen of this already declining species (e.g. Rookmaaker)4 might have contributed as well16. Low genetic diversity in historical samples would provide further support for low population sizes in blue antelope, though this has not been investigated yet. In fact, the knowledge of the blue antelope’s evolutionary history and ecology is very limited and originates from just a few early and, as was common at the time, anecdotal travel reports, the archaeological and paleontological records, and deductions from observations of its extant congeners, the roan (H. equinus) and the sable (H. niger), both of which were described later (in 1803 and 1838, respectively).
The early extinction of the blue antelope is reflected in its scarcity in natural history collections today. Additionally, almost all specimens purported to be of the blue antelope lack secure provenance and are of uncertain taxonomic identity. For more detailed information on provenance and about the specimens in general see Supplementary Document S1. Mohr17, Rookmaaker18 and Renshaw19 collated lists of existing, lost, and potential specimens. To the best of our knowledge, only 16 specimens are recorded as potential blue antelopes in museums (15, if the skull fragment and the mounted skin from Leiden are from the same individual; see "Samples" section). All but one of these are housed in Europe. These comprise four mounted skins (Leiden, Paris, Stockholm, Vienna), six skulls or crania (Berlin, Glasgow, Leiden, Paris), one skull fragment (in Leiden, possibly originating from the mounted skin there), four pairs of horns (Cape Town, London, St Andrews, Uppsala), and one specimen that is either a skull or a pair of horns (in Brussels, currently not accessible due to renovation). Given the morphological similarities with roan and sable antelope and the lack of confirmed reference material, the taxonomic identity of many of these specimens, particularly the skulls, is contentious (e.g. Mohr17, Groves & Westwood)20. This raises the important question: how many of them can truly be assigned to the blue antelope? Several morphological studies have attempted to determine the species identity of these specimens17,20,21, but with unsatisfactory results. Two studies have successfully extracted blue antelope DNA from museum specimens, each working with only a single specimen: Robinson et al.22 analyzed 502 bp of the CYTB gene from the Vienna specimen, and Themudo & Campos23 generated a mitochondrial genome from the Uppsala specimen.
In the present study, we analyzed ten potential blue antelope specimens. We generated a revised complete mitochondrial genome, performed phylogenetic analyses and, in the tradition of Mohr17, Rookmaaker18 and Renshaw19, present a revised list of true blue antelope museum specimens. The genetically confirmed taxonomic identity of these specimens will facilitate morphological research on the blue antelope and reduce the present taxonomic uncertainty. We also present a first preliminary estimate of the genetic diversity of the blue antelope ’museum population’ by comparing two complete and two partial blue antelope mitochondrial genomes.
Material and methods
A thorough museum record and literature search for specimens currently or previously labeled as blue antelopes resulted in a list of 16 potential historical blue antelope specimens (e.g. Mohr17, Rookmaaker18, Husson & Holthuis24, Erdbrink)25: four mounted skins, six skulls/crania, one skull fragment, four pairs of horns, some with frontlet, and one inaccessible specimen that is either a skull or a pair of horns (Table 1, Supplementary Document S1).
All institutions housing specimens were contacted and subsequently ten bone and/or skin samples were obtained. Photographs (if available, Supplementary Figs. S1–S15) and detailed information about the specimens are presented in Supplementary Document S1. Whenever documents have been inspected by one of the authors (for example copies of catalogues), no source is stated; whenever the information was provided by others, this is stated as personal communication.
The specimen from the Swedish Museum of Natural History (Naturhistoriska riksmuseet) in Stockholm (NRM 590107) is a mounted skin of a subadult male, its young age being obvious from its short horns with few rings. The collector A. U. Grill received the specimen from C. P. Thunberg26. In 1829, Grill’s heirs donated it to the Swedish Museum of Natural History17,18. It is highly likely that no skull is inside the skin (see Supplementary Document S1). The mounted skin from the Natural History Museum Vienna (NMW ST 715) is the only known female. Recent X-ray analysis (June 2017) has shown that the Vienna specimen does not contain a skull (Supplementary Fig. S2). According to the acquisition catalogue, it became part of the collection in 1806. It was the first specimen of the species from which DNA was successfully recovered22.
The complete skull (without horn sheaths) from the Hunterian at the University of Glasgow (GLAHM:Z4884) was discovered there in 194921, whereas the complete skull (including both horn sheaths) in the collection of Naturalis Biodiversity Center in Leiden (ZMA.MAM.18623) was formerly stored in the Zoölogisch Museum in Amsterdam before this collection was merged with Naturalis in 2011. To our knowledge, the cranium at the Muséum national d’Histoire naturelle in Paris (MNHN-ZM-AC-1896-100) has not been previously mentioned in the literature. According to the catalogue, it is from Senegal and was donated by a certain Houdelot(?). It was first mentioned in a museum catalogue at the end of the nineteenth century (pers. comm. Joséphine Lésur, in charge of the Collections Ostéologiques d'Anatomie Comparée at the Muséum national d’Histoire naturelle). Two crania and one skull in the Mammal Collection at the Museum für Naturkunde in Berlin were at some point identified as blue antelopes. Only one of these, a cranium (ZMB MAM 8859) was sampled. It is now cataloged as a roan, possibly after Mohr’s17 revision. Its date of arrival in the collection, geographic origin, and sex are unknown.
The skull fragments at Naturalis Biodiversity Center in Leiden consist of the anterior part of a mandible and premaxillary bones (RMNH.MAM.20681.a). They may derive from the same specimen represented also by the mounted skin in this collection (RMNH.MAM.20681.b)24 (see Specimens not analyzed). The collection catalogue from 1887 refers to this as a complete skull24,27, and it may be that the remainder of the skull is within the mounted skin. Therefore, the fragments bear the same object ID as the mounted skin in the collection catalogue, but with ‘b’ for the mounted skin and ‘a’ for the skull fragments. We refer to the skull fragments as Leiden 1 in this study, to distinguish them from the complete skull from Leiden, which is referred to as Leiden 2.
The horns in the Museum of Evolution at the University of Uppsala (UPSZMC 78488) still have traces of fur attached to their bases, but are not connected by a frontlet. From this specimen, we received a fur/skin as well as a bone sample. It had already been used earlier to generate a mitochondrial genome of the blue antelope23. According to Rookmaaker4 it was received in 1781 by C. P. Thunberg from D. F. Immelmann.
The frontlet with horns from the Terrestrial Vertebrate Collection at the Iziko Museums of South Africa in Cape Town (SAM ZM 40759) was first reported by Ozinsky28. The only available information is that it was part of the private collection of Mr. J. Piek from Observatory (Cape Town) and entered the collection in 1989 (pers. comm. Denise Hamerton, curator Terrestrial Vertebrate Collection at Iziko Museums of South Africa). The frontlet with horns from the Bell Pettigrew Museum at the University of St Andrews (BPM 2234) has, to our knowledge, never been mentioned in the literature. It is labeled as ‘Blaubok? Ozanna leucophaeus (Pall.) South Africa, now extinct’. It seems to lack documentation of its history as well as information on its origin.
Specimens not analyzed
The mounted skin at Leiden Naturalis Biodiversity Center (formerly Rijksmuseum van Natuurlijke Historie) (RMNH.MAM.20681.b) is an adult male and the lectotype of the species, to which later Swellendam was assigned as location24. The mounted skin in the Collections d'Anatomie Comparée at the Muséum national d’Histoire naturelle in Paris is an adult male (MNHN-ZM-MO-1994-1103). It was first mentioned in a museum catalogue from the end of the nineteenth century (pers. comm. Joséphine Lésur; for a recent publication see Glenn)29. Mohr17 assumed that the Paris specimen did not contain its skull, on account of the shape of its forehead (where the nasal and frontal bones would be). This was confirmed by Péquignot30. While the Leiden and Paris mounted skins are most likely true blue antelopes (based on their morphological similarity with the genetically confirmed Stockholm and Vienna specimens), despite the comment in Skead31 that a blue antelope could be manufactured ‘using the skin of an animal resembling it’, they should be genetically analyzed in the future.
The Museum für Naturkunde in Berlin houses two more specimens at one time labeled as blue antelopes: the cranium of a female from South Africa (ZMB MAM 8855) and the skull of a male from Sudan (ZMB MAM 8860). Mohr17 determined ZMB MAM 8855 to be a sable after receiving measurements from Berlin, which is probably the reason for its relabeling. ZMB MAM 8860 has to our knowledge never been mentioned in the literature; unfortunately, it was discovered too late to be included in our study.
Little information is available for the frontlet with horns in the Natural History Museum in London (NHMUK GERM 636e). In Lydekker’s32 catalogue of the ungulate mammals in the British Museum it is listed as ‘provisionally referred to this species [blue antelope]’. It was mentioned by Sclater & Thomas10 as having ‘been long in the Museum’. The specimen in the Royal Belgian Institute of Natural Science in Brussels (RBINS 3785) has to our knowledge never been mentioned in the literature and could not be accessed for this study due to collection renovation. According to the museum catalogue, it is either a skull or a pair of horns which was donated to the museum in 1931 by the arachnologist and ichthyologist Dr L. Giltay.
DNA was extracted from bone using the Dabney et al.33 protocol and from skin by using a combination of Rohland et al.34 and Dabney et al.33 protocols with digestion buffer modifications from Taron et al.35 (5 M GuSCN, 25 nM NaCl, 50 mM Tris, 20 mM EDTA, 1% Tween-20, 1% 2-Mercaptoethanol) using columns of Roche’s High Pure Viral Nucleic Acid Kit for purification. DNA extracts were built into single-stranded libraries following Gansauge et al.36 with the adjustment of an initial 15 min. incubation step with 0.5 µl USER (Uracil-Specific Excision Reagent) Enzyme for Uracil removal (modified from Meyer et al.)37. A maximum of 13 ng DNA was used as input for library construction. qPCR was performed to determine the optimal number of amplification cycles for the subsequently performed dual-indexing PCR. Extraction and library blanks were run alongside all samples to check for contamination. For the sample from Uppsala, a library was built from the bone as well as the skin sample. As both the Stockholm and Vienna samples contained very short reads after initial test-sequencing, both were processed on the Pippin Prep (Sage Science) with a 3% Agarose Gel Cassette for targets from 90–250 bp (Marker C) (product no. CSD3010) with selection parameters set to 165–300 bp to remove short reads and thereby improve the mappable fraction of sequenced reads. All pre-PCR lab work was conducted in dedicated archival DNA facilities at the University of Potsdam, Germany. The libraries were shotgun sequenced using custom primers38,39 on an Illumina NextSeq500 at the University of Potsdam generating 75 bp single-end reads.
Mitochondrial genome enrichment
For array capture following Hodges et al.40 and Paijmans et al.41, an Agilent Sure select Array was designed based on the mitochondrial genomes of Hippotragus leucophaeus (NC_03530923), H. equinus (NC_020712)42 and H. niger (NC_020713)42. As H. leucophaeus contained two areas in the control region, between coordinates 15,643–15,673 and 16,396–16,422, with missing/ambiguous data, these were removed from the bait design. For H. niger, one ambiguous base within CYTB was adjusted to match the corresponding position in H. leucophaeus and H. equinus (R, position 14,921). All genomes were divided into 60-mer probes with 3 bp tiling using a custom python script. To avoid underrepresentation of the region where the mitochondrial genome was cut to linearize it, 59 bp from the beginning of each of the mitochondrial genomes were copied to its end. On the same array, mitochondrial genomes for five Caprinae species were present for enrichment of samples from a different project. Prior to capture, libraries were pooled in equimolar amounts according to their mitochondrial endogenous content as determined via shotgun sequencing (Supplementary Table S3 and S4)43. Due to its already high endogenous content, the Stockholm sample was not captured. The capture product was sequenced using custom primers on an Illumina NextSeq500 at the University of Potsdam generating 75 bp single-end reads.
Bioinformatic procedures and analyses
Mitochondrial genome reconstruction
For the reconstruction of the complete mitochondrial genome of the blue antelope, both the Stockholm (NRM 590107) and the Vienna (NMW ST 715) specimens were considered since they are both mounted skins and as such their attribution to the blue antelope is likely correct. However, the Stockholm specimen was chosen as it yielded the best quality DNA (highest endogenous content). For all reads, Illumina adapter sequences (1 bp overlap) and reads < 30 bp were removed with Cutadapt v1.1244. Next, potential PCR-duplicates were removed by sequence identity (--by-seq) with SeqKit v0.12.0 rmdup45 and quality trimming was conducted for a quality of 30 at the 3′ end of the reads with Cutadapt v1.1244. For mitochondrial genome assembly, MITObim v1.9.146,47, which employs the mapper Mira v4.0.248, was used with the --quick option and default settings except for the mismatch value and a limit of 500 iterations. All runs stopped before 500 iterations were reached. Details of the run results are shown in Supplementary Table S6. As reference bait sequences, the complete mitochondrial genomes of the two closest relatives H. niger (NC_020713)42 and H. equinus (NC_020712)42 were used. For each bait, mismatch values from zero to six were tested (Supplementary Table S6). The assembled reads were filtered for a minimum mapping quality of 30, sorted using samtools view and sort v0.1.1949 and read groups were adjusted using Picard AddOrReplaceReadGroups v2.22.0 (Picard Toolkit 2020—http://broadinstitute.github.io/picard/) before duplicates were removed with samtools rmdup v0.1.1949 based on the 5′ mapping coordinate. A consensus sequence was generated for each run using a 75% majority rule threshold for base calling and a minimum coverage of 3x. The consensus sequences were edited such that all started with tRNA-Phe and ended with the control region. The resulting mitochondrial genome differed depending on whether H. niger or H. equinus was used in that 91 bp were only present in the control region when H. niger was used. This could be a bait sequence bias, since there is a region of 78 bp present in the H. niger, but not in the H. equinus reference. Therefore, it could not be determined if this region is present in H. leucophaeus using only these two bait sequences. To infer this, we ran MITObim v1.9.146,47 with single genes, ND4 and CYTB, of H. equinus, H. niger and Capra hircus (KR059146)50 as bait sequences, using the same settings as described before and mismatch values from one to six. The results were treated in the same way as stated above. The complete mitochondrial genome of H. leucophaeus was then generated by aligning the twelve sequences created using H. niger and H. equinus as bait sequences, each with mismatch values from one to six applying the MAFFT algorithm v7.45051,52 with default settings as implemented in Geneious R10 v10.2.353 (https://www.geneious.com). A consensus sequence was generated from this alignment, again employing a 75% majority rule threshold for base calling except for the described area in the control region where only the sequences that used H. niger as bait reference were considered (matching positions 15,676–15,766 in the final sequence). The newly created complete mitochondrial genome of H. leucophaeus was annotated in Geneious R10 v10.2.353 using the available annotated H. niger mitochondrial genome (NC_020713)42.
Data from different sequencing runs were combined per sample before processing. Cutadapt v1.1244 was used to trim Illumina adapter sequences (1 bp overlap) and to discard reads shorter than 30 bp. The resulting reads were mapped to the newly constructed Hippotragus leucophaeus mitochondrial genome and the two available mitochondrial genomes of H. niger and H. equinus from GenBank with the BWA aln algorithm v0.7.8 with default settings54. Quality filtering was performed using samtools view v0.1.1949 applying a minimum mapping quality filter of 30 and a subsequent sorting step with samtools sort v0.1.1949. Duplicates were marked taking both 5′ and 3′ mapping coordinates into account with MarkDupsByStartEnd v0.2.1 (https://github.com/dariober/Java-cafe/tree/master/MarkDupsByStartEnd) and removed with samtools view v0.1.1949.
The reads of each individual were mapped to the complete mitochondrial genomes of the three Hippotragus species H. leucophaeus (this study), H. niger (NC_020713)42 and H. equinus (NC_020712)42 to determine the species identity for each individual. The relative mapping success for each sample was normalized by defining the result of the reference it mapped best to as 1 and dividing the results of each of the other two references by the results of the reference it mapped best to. For each individual, for the reference it mapped best to, a consensus sequence was generated in Geneious R10 v10.2.353 using a 75% majority rule threshold for base calling, a minimum coverage of 3 × and the ‘trim to reference sequence’ option. Positions where an insertion was called relative to the reference were removed if the insertion was covered by less than three reads. To improve the coverage at the edges of the sequences it was necessary to map the obtained reads again to modified versions of the same references. For this, the circular character of the mitochondrial genome was used by cutting the last 100 bp of each reference and concatenating them to the beginning of the sequence to allow reads to map in the region where the reference had been cut before. Consensus sequences were called and insertions removed as described above. Subsequently, the first 100 bp of each sequence were cut and concatenated back to the end of the sequences to match the original reference again. Then the consensus sequences of both mappings were combined using a 50% majority rule threshold for base calling. In a final step, the sequences were edited such that all started with tRNA-Phe and ended with the control region. This resulted in improved sequences for the samples from Glasgow (GLAHM:Z4884), Leiden 1 (RMNH.MAM.20681.a), Berlin (ZMB MAM 8859), Paris (MNHN-ZM-AC-1896-100), St Andrews (BPM 2234), Stockholm (NRM 590107), Uppsala (UPSZMC 78488) and Vienna (NMW ST 715).
An alignment applying the MAFFT algorithm v7.45051,52 to the consensus sequences of the reference that each individual mapped the most base pairs to was built using default parameters as implemented in Geneious R10 v10.2.353 with the gap opening penalty altered to 1.605. In this alignment, the references of H. niger and H. equinus from GenBank were included. Since the new reference of H. leucophaeus is identical to the sample from Stockholm, the reference was not included. As outgroup the mouflon (Ovis aries musimon) was included (HM236184)55. The control region from each sequence was removed from the alignment because this region is challenging to align for divergent sequences. The final alignment (four taxa) was used to generate a maximum-likelihood tree with 100 bootstrap replicates using RAxML 8.2.10 with the GTR + G substitution model (Fig. 3)56.
To rule out the influence of reference bias, a consensus sequence for each sample for each of the three Hippotragus references was generated in Geneious R10 v10.2.353, again using a 75% majority rule threshold for base calling, a minimum coverage of 3 × and the ‘trim to reference sequence’ option. No insertions were deleted and no improvement of the edges of the sequences was performed. The control region was removed. An alignment and a maximum-likelihood tree using RAxML 8.2.10 with GTR + G56 were built separately for the consensus sequences of each of the three references using the parameters described above (Supplementary Figs. S16–S18). The alignments were improved by shifting gaps by hand.
Intraspecific mitochondrial diversity comparison
The consensus sequences of the four specimens identified as blue antelopes (see "Results" section) were aligned using the MAFFT algorithm v7.45051,52 with default parameters as implemented in Geneious R10 v10.2.353. All ambiguities including missing data were removed from the alignment, leaving 6,300 bp. Subsequently, from this alignment a median joining network was built and the nucleotide diversity calculated using POPART v1.757 with default parameters.
Interspecific mitochondrial diversity comparison
The genetic diversity of the blue antelope specimens was estimated with an average pairwise distance (k) approach, where k is the average number of substitutions in a pairwise individual comparison. For comparison, six wild ungulate species with a wide range of characteristics were chosen: one closely related species (scimitar-horned oryx, Oryx dammah), three species that are known to have low genetic diversity, including the European bison (Bison bonasus), the American bison (Bison bison) and the Przewalski’s horse (Equus przewalskii), as well as two species with large geographic ranges, the African buffalo (Syncerus caffer) and the moose (Alces alces). For each of the six comparison species, all sequences considered reliable were downloaded from GenBank. If a sequence was uploaded to GenBank only once, but was found in more than one individual within a study, it was included as many times as individuals with it were present in the respective study (Supplementary Table S5). The control region of each sequence was removed. All sequences were aligned together with the four blue antelope consensus sequences (also without the control region) using the MAFFT algorithm v7.45051,52 with default settings as implemented in Geneious R10 v10.2.353. All positions containing ambiguities/missing data or gaps were excluded from the alignment to ensure that only homologous positions were compared. Subsequently, for each species four sequences were randomly drawn without replacement using seqtk v1.3 (https://github.com/lh3/seqtk), then aligned with MAFFT v7.45351,52 using the default settings for gap opening penalty (--op 1.53) and offset value (--ep 0.123). The pairwise distance was calculated using the command line version of MEGA-CC 1058,59 applying the ‘complete deletion’ option for the treatment of gaps and missing data. This was repeated 1,000 times for each of the species. Finally, the average was calculated using an R script. For the blue antelope, this was performed once with the four available sequences. The results were visualized using RStudio v1.1.42360 (https://www.rstudio.com/) with R v3.6361 (https://www.R-project.org/).
Processing the Stockholm and Vienna samples on the Pippin Prep resulted in 4.5 × more mappable endogenous data for the Stockholm and 13.5 × more for the Vienna sample compared to their respective original libraries. For the mitochondrial genome reconstruction, the results for mismatch values zero contained many unknown bases. Therefore, this value appeared too strict and the results were dismissed. The results using H. niger as assembly bait sequence for mismatch values one and two were identical (both A at position 15,784, C at position 15,786) as well as for mismatch values three to six (R at position 15,784, Y at position 15,786). The same was true when using H. equinus (values 1 & 2: A at position 15,769 and C at position 15,770; values 3–6: R at position 15,769 and Y at position 15,770). One area of 91 bp in the control region was present when using H. niger, but not when using H. equinus as bait sequence. This might be a bait sequence bias since in this area a region of 78 bp is present in H. niger, but not in the H. equinus reference. No run with a single gene as assembly bait sequence resulted in a complete mitochondrial genome. However, the area in question was covered when using CYTB with mismatch values one to six and ND4 with mismatch values four to six, irrespective of the species used as a bait sequence. The results for the area in question were in each case identical to the one obtained when using the complete H. niger sequence as bait.
The complete mitochondrial genome of Hippotragus leucophaeus (Stockholm specimen) is 16,514 bp long and consists of 13 protein coding genes, 22 tRNAs, 2 rRNAs and the control region as expected for a mammalian mitochondrial genome.
For each sample all reads from all runs were combined resulting in 4,751,815—26,107,111 75 bp single end reads (Supplementary Table S2).
Species identity of the museum specimens
The mitochondrial mapping success rates show that the mounted skins from Stockholm (NRM 590107) and Vienna (NMW ST 715), the skull fragments from Leiden 1 (RMNH.MAM.20681.a) and the pair of horns from Uppsala (UPSZMC 78488) are conspecific. Since Leiden 1 is probably part of the skull of the blue antelope lectotype specimen and the Stockholm and Vienna mounts are blue antelopes beyond reasonable doubt based on their morphology, these four specimens can be attributed to Hippotragus leucophaeus (Fig. 2, Supplementary Table S2).
The specimens from Paris (MNHN-ZM-AC-1896-100, skull), Berlin (ZMB MAM 8859) and St Andrews (BPM 2234), however, belong to roan (H. equinus), while those from Glasgow (GLAHM:Z4884), Leiden 2 (ZMA.MAM.18623) and Cape Town (SAM ZM 40759) are sable (H. niger) (Fig. 3, Table 1).
All four blue antelope samples map second best to the sable and all sable specimens map second best to the blue antelope mitochondrial genome. On the other hand, all roan samples map almost equally well to the sable and blue antelope mitochondrial genomes, with a slightly higher value for the blue antelope (Fig. 2).
Complete mitochondrial genomes were generated for Stockholm (104x) and Uppsala (17.7x), and partial mitochondrial genomes were generated for Leiden 1 (3.9x), Vienna (6.2x), Berlin (5.1x), Paris (7.3x), St Andrews (13.7x), Cape Town (2.2x), Glasgow (4.1x) and Leiden 2 (1.7x) (Supplementary Table S7).
The maximum-likelihood phylogeny groups Stockholm (NRM 590107), Vienna (NMW ST 715), Leiden 1 (RMNH.MAM.20681.a) and Uppsala (UPSZMC 78488) together as blue antelopes; Glasgow (GLAHM:Z4884), Leiden 2 (ZMA.MAM.18623) and Cape Town (SAM ZM 40759) with the sable reference; and Paris (MNHN-ZM-AC-1896-100), Berlin (ZMB MAM 8859) and St Andrews (BPM 2234) with the roan reference (Fig. 3). All three clades have 100% bootstrap support. The possibility of a reference bias could be excluded as each of the three maximum-likelihood trees using the same mapping reference for each specimen confirms the above relationships (Supplementary Fig. S16-18).
Since the identity of all tested samples could be clearly established, this allowed for a tentative estimate of the genetic diversity of the blue antelope museum specimens.
Low levels of genetic diversity in blue antelope museum specimens
The comparison of the four unambiguous blue antelope specimens using a median joining network, taking only the positions into account where all specimens had unambiguous available data and including the control region, revealed only six segregating sites (Fig. 4) and a nucleotide diversity (pi) of 0.0005. The sequences of the Stockholm and Uppsala specimens were identical in this comparison.
In the pairwise distance comparison, the blue antelope sequences from Stockholm, Vienna, Uppsala and Leiden 1 were compared. The resulting k value was compared to the k values of 1,000 comparisons of four randomly chosen sequences of homologous positions of six wild ungulate species (Fig. 5). In comparison to the other species, the blue antelope shows a rather modest k value (3.2), similar to that in the American bison.
Our results show that only four of the ten analyzed specimens are in fact blue antelopes, while the remaining six belong to either roan or sable. The mapping success per reference species (Fig. 2) together with the well-resolved phylogeny (Fig. 3) yield unequivocal evidence as to the species identity of each analyzed specimen. The pattern that all sable map second best to the blue antelope mitochondrial genome and all blue antelopes map second best to the sable mitochondrial genome (Fig. 2) is in accordance with our phylogeny (Fig. 3) and previous results, indicating that the blue and sable antelope are sister species to the exclusion of the roan23.
Our results suggest that historical specimens of the blue antelope in museum collections are even rarer than previously thought (although fossil remains are more abundant, see below). Further work should examine the six remaining potential blue antelope specimens not analyzed here, although two of these are currently listed as sable (ZMB MAM 8855) and roan (ZMB MAM 8860), respectively. The blue antelope is therefore among the rarest historically extinct large mammal species in museums. By comparison, the other recently extinct South African ungulate, the quagga (Equus quagga quagga), a subspecies of the plains zebra, is represented by ~ 34 individual specimens62,63, and of Steller’s sea cow (Hydrodamalis gigas), which became extinct roughly at the same time as the blue antelope, there are at least 27 skeletons, 62 additional skulls and more than 550 bones64.
Since our study only analyzed mitochondrial DNA, we cannot exclude the possibility that some of our sampled specimens are hybrids. The roan had overlapping distributions with the blue antelope since at least the Last Glacial Maximum5,65, and potentially longer. In historical times Du Plessis66 found no evidence of roan antelope as far south as the Cape Floristic Region, but Mohr17 considered a sketch by R. J. Gordon from 1778 near Plettenberg Bay to be more likely of a roan than a blue antelope. This specimen is considered to be the holotype of the roan by Grubb67. This would make this the last roan to be documented in the southern Cape before its extirpation in that region (yet undescribed as a species)17,65. However, population level nuclear DNA data from the blue antelope, which are not currently available, and from species it might have hybridized with, would be required to investigate whether any of the blue antelope museum specimens represent hybrids.
Osteological material, especially in the form of skulls and teeth, is extraordinarily important for comparative morphological, morphometric and taxonomic studies. It is widely used as reference material for museum specimens and archaeological and paleontological material to study and delineate species. For the blue antelope Groves & Westwood20 stated that ‘The authentication of even one skull of this extinct antelope would be a significant event.’ With the only historical osteological remains of the blue antelope represented by the skull fragments in Leiden, the horns in Uppsala, and some phalanges within the Vienna mounted skin, our results suggest that there is currently not a single skull that could be used as a reference against which to evaluate historical or fossil specimens. This creates the problem whereby archaeological and paleontological specimens (mostly teeth) identified as blue antelope through morphological characters (namely distinguished from roan by smaller molars and premolars, and from sable by larger premolars)5,65 cannot be directly compared with the historical skins, horns and bone fragments identified as blue antelope through DNA analyses. This difficulty is further demonstrated by the many misidentified skulls and frontlets presented in our study, which is a known issue in museum collections68. This means that, while the fossil and historical specimens assigned to the blue antelope are very likely one and the same species, this cannot be directly demonstrated. Non-invasive imaging technologies like X-ray or µCT should be applied to investigate whether the Leiden mounted skin possesses a complete (or partial) skull. Ultimately, if a skull is present, it could be scanned, and a cast could be produced by means of a 3D printer. The same could be done for the Stockholm specimen to be certain that it really does not contain a skull.
With only four to maximally ten blue antelope specimens existing, they should be highly valued in museum collections. Since misidentification can go both ways, it is also possible that further specimens of the blue antelope exist, but are mislabeled as sable or roan. This is especially true in light of the fact that their status as separate species was not settled for quite some time10,69 and that due to its early extinction, the blue antelope was never well known. Further blue antelope specimens might be privately owned in South Africa or elsewhere. For now, the genetic analysis of known potential blue antelope specimens in collections should be prioritized to perhaps increase the number of unequivocal individuals of this iconic extinct mammal species.
Our sample size is too small to draw well-founded conclusions about the genetic diversity of the blue antelope population in the seventeenth and eighteenth centuries. However, our results suggest that the blue antelope exhibited low genetic diversity in historical times, as previously suspected16,22, similar to the low levels seen in the European70 and American bison71. Low genetic diversity itself does not necessarily lead to extinction72, but it can render species more susceptible to diseases73,74,75,76. However, there is no evidence that the blue antelope was affected in this way. Rather, low genetic diversity itself is likely to be an indication of low population size, and this would certainly have made the blue antelope much more susceptible to extinction in the face of hunting or environmental disturbance, as suggested by Kerley et al.16 and Faith & Thompson6.
Of the four confirmed blue antelope specimens, all lack verified, detailed location information. Hence, we cannot draw conclusions concerning their geographic origin. However, the two specimens from Swedish museums—Stockholm and Uppsala—have most likely identical mitochondrial genomes, suggesting that they might have originated from the same herd. This seems likely considering that both were acquired by C. P. Thunberg, who was in charge of the collection in Uppsala at the time.
For a better estimate of the genetic diversity of the blue antelope in the seventeenth and eighteenth centuries, larger sample sizes would be needed. For now, this is not feasible since there is an insufficient number of potential blue antelope specimens that remain to be tested. However, there are large numbers of archaeological and paleontological specimens attributed to this species from late Pleistocene and Holocene sites in the southern and western Cape region7, with which ancient DNA analyses can be carried out to address questions of past population size changes.
There is an interesting parallel to the bontebok (Damaliscus pygargus pygargus) that had a similar historical distribution and was also endemic to the Cape Floristic Region15,66,77. Like the blue antelope, the bontebok is thought to have been severely impacted by hunting and pastoralism, resulting in fragmented populations, bringing the species close to extinction at the beginning of the nineteenth century1,78. Its genetic diversity is considered to be low today79, and its survival is only thanks to the efforts of private landowners who enclosed some of the remaining animals1. Unfortunately, the blue antelope went extinct before similar measures could be taken.
The blue antelope was likely one of the inhabitants of the Palaeo-Agulhas plain, the coastal platform off the southern Cape that was exposed during marine regressions (glacials) and provided a nutrient-rich ecosystem that supported diverse ungulate communities. However, during high sea levels (interglacials), the inhabitants would have been restricted to the nutrient-poor and therefore suboptimal fynbos habitats80,81,82,83,84 where they might have undergone population fragmentation6,84. On the other hand, the blue antelope (like other species) clearly survived such Pleistocene climatic fluctuations without going extinct6,84,85. Kerley et al.16, based on historical sightings, estimated a total population size of as few as 370 individuals in only a single population at the time of the arrival of the European colonists, which would have rendered the species already highly threatened6,84,85. Therefore, it seems likely that other factors must have contributed to its demise in historical times. Resource competition with livestock, habitat deterioration in addition to a suboptimal and probably fragmented habitat likely put the remaining blue antelope population under extreme pressure at the time of European colonization6,84. Unsustainable hunting and further habitat transformation at the time would have been the last contributing piece that led to the extinction of the species84.
We show that the blue antelope is not only blue but also lonesome, with only four unequivocal historical specimens in collections today: Stockholm and Vienna (mounted skins), Leiden (skull fragments) and Uppsala (pair of horns). The mounted skins from Leiden and Paris (although the former is probably from the same individual as the skull fragments) can be considered blue antelopes as well. In addition, there are four more potential specimens (in Berlin, Brussels and London). This makes it one of the scarcest historical mammal species in museums, with currently no skull identified that could serve as a comparative morphological reference. Our study is yet another example that misidentifications can be an issue in museum collections, which may seriously impact morphological studies. It highlights the promising potential of the application of archival DNA to resolve existing uncertainties of museum specimens. Furthermore, our preliminary assessment hints at a rather low level of mitochondrial diversity within the blue antelope ‘museum population’.
All supplementary material (Supplementary Information/Document S1 and Supplementary Data 1–6) including alignments can be downloaded from the journal’s website at https://doi.org/10.1038/s41598-020-80142-2. All complete and partial mitochondrial genomes were uploaded to GenBank under the accession numbers MW222233-MW222234 and MW228401-MW228408.
FitzSimons, F. W. The bluebuck or blaauwbok (Hippotragus leucophaeus). In The Natural History of South Africa Vol. 3 97–105 (Longmans, Green and Co., London, 1920).
Harper, F. Blaauwbok; blue-buck. In Extinct and Vanishing Mammals of the Old World 698–700 (The Lord Baltimore Press, Baltimore, 1945).
Skead, C. J. Blue antelope (extinct blaauwbok), Hippotragus leucophaeus (Pallas, 1766). In Historical Mammal Incidence in the Cape Province vol. 1 526–537 (Department of Nature and Environmental Conservation of the Provincial Administration of the Cape of Good Hope, 1980).
Rookmaaker, L. C. The Zoological Exploration of Southern Africa 1650–1790 (A. A. Balkema, Rotterdam, 1989).
Klein, R. G. On the taxonomic status, distribution and ecology of the blue antelope, Hippotragus leucophaeus (Pallas, 1766). Ann. S. Afr. Mus. 65, 99–143 (1974).
Faith, J. T. & Thompson, J. C. Fossil evidence for seasonal calving and migration of extinct blue antelope (Hippotragus leucophaeus) in southern Africa. J. Biogeogr. 40, 2108–2118 (2013).
Avery, D. M. A Fossil History of Southern African Land Mammals (Cambridge University Press, Cambridge, 2019).
Plug, I. Late Pleistocene and Holocene hunter–gatherers in the eastern highlands of South Africa and Lesotho: a faunal interpretation. J. Archaeol. Sci. 24, 715–727 (1997).
Pallas, P. S. Miscellanea Zoologica Quibus Novae Imprimis Atque obscurae Animalium Species Describuntur (Petrum van Cleef, Den Haag, 1766).
Sclater, P. L. & Thomas, O. The blue-buck. In The Book of Antelopes Vol. 4 5–12 (R. H. Porter, London, 1899).
Schreyer, J. Neue Ost-Indianische Reiß-Beschreibung (Johann Christian Wohlfahrt, Leipzig, 1681).
Kolb, P. Caput Bonae Spei hodiernum (Peter Conrad Monath, Nürnberg, 1719).
Lichtenstein, H. Reisen im südlichen Africa in den Jahren 1803, 1804, 1805 und 1806 (C. Salfeld, Berlin, 1811).
Lichtenstein, H. Die Gattung Antilope. Ges. Naturf. Freunde Berlin Mag. neuesten Entdeck. gesammten Naturk. 6, 147–160, 163–182 (1814).
Klein, R. G. Palaeoenvironmental implications of quaternary large mammals in the fynbos region. In Fynbos Paleoecology: A Preliminary Synthesis (eds. Deacon, H. J., Hendrey, Q. B. & Lambrechts, J. N. N.) 116–138 (CSIR, Pretoria, 1983).
Kerley, G. I. H., Sims-Castley, R., Boshoff, A. F. & Cowling, R. M. Extinction of the blue antelope Hippotragus leucophaeus: modeling predicts non-viable global population size as the primary driver. Biodivers. Conserv. 18, 3235–3242 (2009).
Mohr, E. Der Blaubock Hippotragus leucophaeus (Pallas, 1766)—Eine Dokumentation (Paul Parey, Hamburg, 1967).
Rookmaaker, L. C. Additions and revisions to the list of specimens of the extinct blue antelope (Hippotragus leucophaeus). Ann. S. Afr. Mus. 102, 131–141 (1992).
Renshaw, G. The blaauwbok. Natural History Essays 38–58 (Sherrat & Hughes, London, 1904).
Groves, C. P. & Westwood, C. R. Skulls of the blaauwbok Hippotragus leucophaeus. Z. Säugetierkd. 60, 314–318 (1995).
Broom, R. The extinct blue buck of South Africa. Nature 164, 1097–1098 (1949).
Robinson, T. J., Bastos, A. D., Halanych, K. M. & Herzig, B. Mitochondrial DNA sequence relationships of the extinct blue antelope Hippotragus leucophaeus. Naturwissenschaften 83, 178–182 (1996).
Themudo, G. E. & Campos, P. F. Phylogenetic position of the extinct blue antelope, Hippotragus leucophaeus (Pallas, 1766) (Bovidae: Hippotraginae), based on complete mitochondrial genomes. Zool. J. Linn. Soc. 182, 225–235 (2017).
Husson, A. M. & Holthuis, L. B. On the type of Antilope leucophaea Pallas, 1766, preserved in the collection of the Rijksmuseum van Natuurlijke Historie Leiden. Zool. Meded. 44, 147–157 (1969).
Erdbrink, D. P. B. Protoryx from three localities East of Maragheh, N.W. Iran. Proc. Kon. Ned. Akad. Wet. B 91, 101–159 (1988).
Lindroth, P., Gustavo. D.D. Museum Naturalium Grillium Soderforssiense (A.J. Nordstrom, Stockholm, 1788).
Jentink, F. A. Aegocerus. In Catalogue Ostéologique des Mammifères 135 (1887).
Ozinsky, S. Rare blue antelope horns found. Sagittarius 4, 31 (1989).
Glenn, I. The Paris bloubok (Hippotragus leucophaeus (Pallas, 1766) [Bovidae]) and its provenance. Zoosystema 42, 77–84 (2020).
Péquignot, A. The history of taxidermy: clues for preservation. Collections 2, 245–255 (2006).
Skead, C. J. Blue antelope (or extinct blaauwbok, bloubok), Hippotragus leucophaeus (Pallas, 1776). In Historical Mammal Incidence in the Cape Province vol. 2 631–634 (The Chief Directorate Nature and Environmental Conservation of the Provincial Administration of the Cape of Good Hope, 1987).
Lydekker, R. Catalogue of the Ungulate Mammals in the British Museum (Natural History) Vol. 3 (British Museum (Natural History), London, 1914).
Dabney, J. et al. Complete mitochondrial genome sequence of a Middle Pleistocene cave bear reconstructed from ultrashort DNA fragments. PNAS 110, 15758–15763 (2013).
Rohland, N., Siedel, H. & Hofreiter, M. Nondestructive DNA extraction method for mitochondrial DNA analyses of museum specimens. Biotechniques 36, 814–821 (2004).
Taron, U. H., Lell, M., Barlow, A. & Paijmans, J. L. A. Testing of alignment parameters for ancient samples: evaluating and optimizing mapping parameters for ancient samples using the TAPAS tool. Genes 9, 157 (2018).
Gansauge, M.-T. et al. Single-stranded DNA library preparation from highly degraded DNA using T4 DNA ligase. Nucleic Acids Res. 45, e79 (2017).
Meyer, M. et al. A high-coverage genome sequence from an archaic Denisovan individual. Science 338, 222–226 (2012).
Gansauge, M.-T. & Meyer, M. Single-stranded DNA library preparation for the sequencing of ancient or damaged DNA. Nat. Protoc. 8, 737–748 (2013).
Paijmans, J. L. A. et al. Sequencing single-stranded libraries on the Illumina NextSeq 500 platform. Preprint at: http://arxiv.org/abs/1711.11004 (2017).
Hodges, E. et al. Hybrid selection of discrete genomic intervals on custom-designed microarrays for massively parallel sequencing. Nat. Protoc. 4, 960–974 (2009).
Paijmans, J. L. A., Gloria, G. F. & Förster, D. W. Application of solid-state capture for the retrieval of small-to-medium sized target loci from ancient DNA. In Ancient DNA—Methods and Protocols (eds. Shapiro, B. et al.) 129–139 (Humana Press, New York, 2019).
Hassanin, A. et al. Pattern and timing of diversification of Cetartiodactyla (Mammalia, Laurasiatheria), as revealed by a comprehensive analysis of mitochondrial genomes. C. R. Biol. 335, 32–50 (2012).
Paijmans, J. L. A. et al. Ancestral mitogenome capture of the Southeast Asian banded linsang. PLoS ONE 15, e0234385 (2020).
Martin, M. Cutadapt removes adapter sequences from high-throughput sequencing reads. EMBnet.journal 17, 10–12 (2011).
Shen, W., Le, S., Li, Y. & Hu, F. SeqKit: A cross-platform and ultrafast toolkit for FASTA/Q file manipulation. PLoS ONE 11, e0163962 (2016).
Hahn, C., Bachmann, L. & Chevreux, B. Reconstructing mitochondrial genomes directly from genomic next-generation sequencing reads—a baiting and iterative mapping approach. Nucleic Acids Res. 41, e129 (2013).
Hahn, C. Assembly of ancient mitochondrial genomes without a closely related reference sequence. In Ancient DNA—Methods and Protocols (eds. Shapiro, B. et al.) 195–213 (Humana Press, New York, 2019).
Chevreux, B., Wetter, T. & Suhai, S. Genome Sequence Assembly Using Trace Signals and Additional Sequence Information. Computer Science and Biology: Proceedings of the German Conference on Bioinformatics (GCB) 99, 45–56 (1999).
Li, H. et al. The sequence alignment/map format and SAMtools. Bioinformatics 25, 2078–2079 (2009).
Colli, L. et al. Whole mitochondrial genomes unveil the impact of domestication on goat matrilineal variability. BMC Genom. 16, 1115 (2015).
Katoh, K., Misawa, K., Kuma, K. & Miyata, T. MAFFT: a novel method for rapid multiple sequence alignment based on fast fourier transform. Nucleic Acids Res. 30, 3059–3066 (2002).
Katoh, K. & Standley, D. M. MAFFT Multiple sequence alignment software version 7: improvements in performance and usability. Mol. Biol. Evol. 30, 772–780 (2013).
Kearse, M. et al. Geneious basic: an integrated and extendable desktop software platform for the organization and analysis of sequence data. Bioinformatics 28, 1647–1649 (2012).
Li, H. & Durbin, R. Fast and accurate short read alignment with Burrows-Wheeler transform. Bioinformatics 25, 1754–1760 (2009).
Meadows, J. R. S., Hiendleder, S. & Kijas, J. W. Haplogroup relationships between domestic and wild sheep resolved using a mitogenome panel. Heredity (Edinb.) 106, 700–706 (2011).
Stamatakis, A. RAxML version 8: a tool for phylogenetic analysis and post-analysis of large phylogenies. Bioinformatics 30, 1312–1313 (2014).
Leigh, J. W. & Bryant, D. POPART: full-feature software for haplotype network construction. Methods Ecol. Evol. 6, 1110–1116 (2015).
Kumar, S., Stecher, G., Peterson, D. & Tamura, K. MEGA-CC: computing core of molecular evolutionary genetics analysis program for automated and iterative data analysis. Bioinformatics 28, 2685–2686 (2012).
Kumar, S., Stecher, G., Li, M., Knyaz, C. & Tamura, K. MEGA X: molecular evolutionary genetics analysis across computing platforms. Mol. Biol. Evol. 35, 1547–1549 (2018).
RStudio Team. RStudio: Integrated Development for R. (RStudio, Inc., Boston, 2016).
R Core Team. R: A Language and Environment for Statistical Computing (R Foundation for Statistical Computing, Vienna, 2019).
Rau, R. E. Revised list of the preserved material of the extinct cape colony quagga, Equus quagga quagga (Gmelin). Ann. S. Afr. Mus. 65, 41–87 (1974).
Rau, R. E. Additions to the revised list of preserved material of the extinct Cape Colony quagga and notes on the relationship and distribution of southern plains zebras. Ann. S. Afr. Mus. 77, 27–45 (1978).
Mattioli, S. & Domning, D. P. An annotated list of extant skeletal material of Steller’s sea cow (Hydrodamalis gigas) (Sirenia: Dugongidae) from the Commander Islands. Aquat. Mam. 32, 273–288 (2006).
Faith, J. T. Conservation implications of fossil roan antelope (Hippotragus equinus) in Southern Africa’s Cape Floristic Region. In Paleontology in Ecology and Conservation (ed. Louys, J.) 239–251 (Springer, Berlin, 2012).
du Plessis, S. F. The Past and Present Geographical Distribution of the Perissodactyla and Artiodactyla in Southern Africa (University of Pretoria, Pretoria, 1969).
Grubb, P. Types and type localities of ungulates named from southern Africa. Koedoe 42, 13–45 (1999).
Kitchener, A. C., Machado, F. A., Hayssen, V., Moehlman, P. D. & Viranta, S. Consequences of the misidentification of museum specimens: the taxonomic status of Canis lupaster soudanicus. J. Mammal. https://doi.org/10.1093/jmammal/gyaa080 (2020).
Kohl, F. F. Ueber neue und seltene Antilopen des k. k. naturhistorischen Hofmuseums. Ann. K. K. Naturh. Hofmus. Wien 1, 75–86 (1886).
Węcek, K. et al. Complex admixture preceded and followed the extinction of wisent in the wild. Mol. Biol. Evol. 34, 598–612 (2016).
Douglas, K. C. et al. Complete mitochondrial DNA sequence analysis of Bison bison and bison–cattle hybrids: function and phylogeny. Mitochondrion 11, 166–175 (2011).
Tokarska, M., Pertoldi, C., Kowalczyk, R. & Perzanowski, K. Genetic status of the european bison Bison bonasus after extinction in the wild and subsequent recovery. Mammal. Rev. 41, 151–162 (2011).
Lacy, R. C. Importance of genetic variation to the viability of mammalian populations. J. Mammal. 78, 320–335 (1997).
O’Brien, S. J. et al. Genetic basis for species vulnerability in the cheetah. Science 227, 1428–1434 (1985).
O’Brien, S. J. & Evermann, J. F. Interactive influence of infectious disease and genetic diversity in natural populations. Trends Ecol. Evol. 3, 254–259 (1988).
Coltman, D. W., Pilkington, J. G., Smith, J. A. & Pemberton, J. M. Parasite-mediated selection against inbred soay sheep in a free-living, island population. Evolution 53, 1259–1267 (1999).
Kerley, G. I. H., Pressey, R. L., Cowling, R. M., Boshoff, A. F. & Sims-Castley, R. Options for the conservation of large and medium-sized mammals in the Cape Floristic Region hotspot South Africa. Biol. Conserv. 112, 169–190 (2003).
van der Merwe, N. J. Die Bontebok. Koedoe 11, 161−168 (1968).
van Wyk, A. M., Kotzé, A., Randi, E. & Dalton, D. L. A hybrid dilemma: a molecular investigation of South African bontebok (Damaliscus pygargus pygargus) and blesbok (Damaliscus pygargus phillipsi). Conserv. Genet. 14, 589–599 (2013).
Marean, C. W. et al. Stone Age people in a changing South African Greater Cape Floristic Region. In Fynbos: Ecology, Evolution, and Conservation of a Megadiverse Region (eds. Allsopp, N., Colville, J. F. & Verboom, G. A.) 164–199 (Oxford University Press, Oxford, 2014).
Copeland, S. R. et al. Strontium isotope investigation of ungulate movement patterns on the Pleistocene Paleo-Agulhas Plain of the Greater Cape Floristic Region South Africa. Quat. Sci. Rev. 141, 65–84 (2016).
Cawthra, H. C., Cowling, R. M., Andò, S. & Marean, C. W. Geological and soil maps of the Palaeo-Agulhas Plain for the Last Glacial Maximum. Quat. Sci. Rev. 235, 105858 (2020).
Cowling, R. M. et al. Describing a drowned Pleistocene ecosystem: Last Glacial Maximum vegetation reconstruction of the Palaeo-Agulhas Plain. Quat. Sci. Rev. 235, 105866 (2020).
Venter, J. A., Brooke, C. F., Marean, C. W., Fritz, H. & Helm, C. W. Large mammals of the Palaeo-Agulhas Plain showed resilience to extreme climate change but vulnerability to modern human impacts. Quat. Sci. Rev. 235, 106050 (2020).
Klein, R. G. The large mammals of southern Africa: Late Pliocene to recent. In Southern African Prehistory and Paleoenvironments 107–146 (A. A. Balkema, Rotterdam, 1984).
This work was supported by the Deutsche Forschungsgemeinschaft (DFG, German Research Foundation) project number 315696891 to M.H. and F.B. (HO 3492/3-1, BI 1879/2-1). We acknowledge the support of Iziko South African Museums, Heritage Western Cape, Cape Nature and South African Heritage Resources Agency. We are grateful to Frieder Mayer, Steffen Bock, Christiane Funk and Detlef Willborn (Museum für Naturkunde, Berlin), Maggie Reilly (University of Glasgow), Denise Hamerton and Jofred Opperman (Iziko South African Museums), Joséphine Lésur (Muséum national d’Histoire naturelle), Carl Smith and Claire Phillips (University of St Andrews) and Hans Mejlon (University of Uppsala) for contributing samples to this study, providing sample information and/or sample photographs. For the latter two we would also like to thank Olivier S. G. Pauwels (Royal Belgian Institute of Natural Sciences), Roberto Portela Miguez (The Natural History Museum) and Carina Phillips (Royal College of Surgeons). We would also like to thank Felix C. Staeps for writing an R script for the diversity comparison. We are grateful to Graham I. H. Kerley and Jan Robovsky for helpful and constructive reviews of an earlier version of this manuscript.
The authors declare no competing interests.
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Hempel, E., Bibi, F., Faith, J.T. et al. Identifying the true number of specimens of the extinct blue antelope (Hippotragus leucophaeus). Sci Rep 11, 2100 (2021). https://doi.org/10.1038/s41598-020-80142-2
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