Two lineages of bivalve transmissible neoplasia (BTN), BTN1 and BTN2, are known in blue mussels Mytilus. Both lineages derive from the Pacific mussel M. trossulus and are identified primarily by their unique genotypes of the nuclear gene EF1α. BTN1 is found in populations of M. trossulus from the Northeast Pacific, while BTN2 has been detected in populations of other Mytilus species worldwide but not in M. trossulus itself. Here we examined M. trossulus from the Sea of Japan (Northwest Pacific) for the presence of BTN. Using hemocytology and flow cytometry of the hemolymph, we confirmed the presence of disseminated neoplasia in our specimens. Cancerous mussels possessed the BTN2 EF1α genotype and two mitochondrial haplotypes with different recombinant control regions, similar to that of common BTN2 lineages. This is the first report of BTN2 in its original host species M. trossulus. A comparison of all available BTN and M. trossulus COI sequences suggests a common and recent origin of BTN2 diversity in populations of M. trossulus outside the Northeast Pacific, possibly in the Northwest Pacific.
Clonally transmissible cancer (CTC) is a neoplastic disease passed from individual to individual by physical transfer of cancer cells1,2,3. The first inkling of a transmissible cancer came from a study of canine transmissible venereal tumor, CTVT, dating back to 18764. Since then CTC has been confirmed for CTVT5 and the facial tumor of Tasmanian devil Sarcophilus harrisii6,7 and, more recently, for several lineages of disseminated neoplasia (DN) of six marine bivalve mollusks: Mya arenaria8, Cerastoderma edule, Polititapes aureus, Mytilus trossulus2, Mytilus edulis9 and Mytilus chilensis10.
A straightforward method of CTC diagnostics is DNA genotyping. The genotype of CTC cancer cells is different from that of the host cells. The result is genetic chimerism, when an individual possesses cells with different genotypes9. At the same time, cancer cells of the same lineage have the same genotype in different infected individuals. Such lineage-specific genotypes are thought to derive from the “patient zero”, the host individual in which the cancer originated2,8,11,12.
The finding that CTC is the cause of DN in six different bivalve species is fairly recent, and it is reasonable to anticipate that further discoveries will turn up. There are also other lines of indirect evidence pointing to a widespread occurrence of transmissible cancers in bivalves13. At the same time, the data are not sufficient to ensure that CTC is the only cause of DN in those six species, or whether CTC is the usual cause of DN in bivalves in general.
DN is a fatal leukemia-like cancer affecting many marine bivalves14. It was first described in M. trossulus from the Northeast Pacific almost half a century ago15. DN is manifested in an uncontrolled proliferation of neoplastic cells in the hemolymph16, which ultimately replace healthy hemocytes. To note, though neoplastic cells are usually also referred to as hemocytes, their tissue origin remains unknown14,17.
Normal hemocytes of healthy bivalves (agranulocytes and granulocytes) are diploid and have a low mitotic activity18,19. Neoplastic hemocytes are aneuploid18,19,20,21,22, and have a high proliferation rate and a striking morphology. They are rounded, with a high nucleus-to-cytoplasm ratio14,22,23, and their nucleus is pleomorphic (i.e. variable in shape) and larger than that of normal hemocytes. As the disease progresses, the proliferating cells infiltrate other tissues, which leads to the loss of integration and normal functioning of organs24,25. DN may reach an epizootic level, causing mass mortality in wild and commercial bivalve populations14,22,24.
There are two approaches to DN diagnostics. The first approach is based on direct examination of cells in hemolymph smears or tissue sections. Various hemocytological techniques may be employed such as light microscopy of fresh or stained hemolymph smears26,27, microscopy of hemocytes with monoclonal antibodies specific to neoplastic cells28, and immunochemistry with antibodies specific to mitotic spindles (for revealing proliferating cells)29. The second approach is based on measuring DNA content. It employs flow cytometry of hemocytes labeled with fluorescent dyes specifically binding DNA19. Flow cytometry is less sensitive to the initial stages of DN than hemocytology but allows an efficient examination of large samples19,22.
Smooth‐shelled blue mussels of the Mytilus edulis species complex are widely distributed in cold-temperate seas of both the Northern (M. edulis, M. trossulus, M. galloprovincialis) and the Southern (M. galloprovincialis, M. chilensis, M. platensis and M. planulatus) Hemispheres30,31. Mussels have been reported to harbor two presumably independent CTC lineages, BTN1 and BTN210 (here BTN stands for bivalve transmissible neoplasia). Both lineages have been derived from M. trossulus, i.e. they have its genome. They are marked by different alleles of mitochondrial and nuclear loci, and the best single marker to distinguish the two lineages from each other and from hosts being the gene coding the elongation factor one alpha (EF1α)2,10. BTN1 was described in populations of its original host species in British Columbia (Northeast Pacific). BTN2 in turn has so far been found in M. edulis from Western Europe (Northeast Atlantic), in M. chilensis from Southern Chile (Southeast Pacific) and from the Beagle Channel in Argentina (Southwest Atlantic), but not in M. trossulus itself2,10. Yonemitsu et al.10 suggested that the original host, M. trossulus, could have evolved resistance to BTN2. Mitochondrial genomes of BTN2 clones from Chilean M. chilensis have been reported to be the product of recombination between the cancer (i.e. M. trossulus-derived) and the host (M. chilensis) mitogenome10.
So, M. trossulus gave rise to at least two CTCs, BTN1 and BTN2. BTN2 is a cross-species cancer, which is supposedly prone to occasional mitochondrial capture from the transient host and subsequent mitochondrial DNA recombination between the cancer and the host. Taken individually, these features are not unique. Two independent lineages of the facial tumor affecting Tasmanian devils are known32. Neoplastic hemocytes in the bivalve P. aureus have the genotype of another bivalve, Venerupis corrugata, for which CTC has not been reported2. Multiple episodes of mitochondrial capture from hosts and recombination between cancer and host mitogenomes are confirmed for CTVT33.
The total geographical distribution of BTN in the circum-global M. edulis complex remains poorly characterized, also as regards the original host species M. trossulus. M. trossulus is basically a North Pacific species, which then has spread to many areas of the North Atlantic in a series of repeated invasions34,35,36. In the Pacific it is distributed from the Arctic to the Gulf of California along the North American coast and to the Sea of Japan (hereinafter, SOJ) along the Asian coast30. So far only American Pacific populations of M. trossulus have been screened for BTN2. Riquet et al.9 and Yonemitsu et al.10 compared BTN mitochondrial sequences with all publically available M. trossulus sequences. Considering the common properties of sequences derived from BTN2, from a mussel individual 62mc10 of M. trossulus from the Baltic Sea (NCBI accession number KM19213337) and individuals from Norway38, Yonemitsu et al.10 hypothesized that the BTN2 lineage originated in a North European M. trossulus population, i.e. outside of the ancestral range of this species. DN has indeed been recorded in M. trossulus in the Baltic Sea39. However, DN was also found in the SOJ40, within the ancestral range of M. trossulus where the presence of BTN has so far not been assessed. In the Northeast Pacific, on the North American coast, mussels are infected with BTN1, but the possible occurrence and identity of the infections on the opposite side of the Ocean are unknown.
The aim of our study was to examine the populations of M. trossulus from the SOJ for the presence of BTN and, should it be found, to establish its genetic affinity with the known BTN lineages.
Material and methods
The workflow of the study is depicted in Fig. 1. In brief, mussels were collected in the Gulf of Peter the Great, the SOJ. Different tissues were sampled from each individual (“Sample collection and preprocessing” step). The hemolymph of all mussels was analyzed by flow cytometry. Based on the results, the mussels were preliminary classified as cancerous (DN-suggested) if an increased fraction of aneuploid hemocytes was registered. For five mussels (four DN-suggested and a healthy control) the diagnosis was verified by direct examination of hemocytes using hemocytology and immunochemistry (“DN diagnostics”). The same cancerous mussels and the controls were used during the next steps. There, we generally followed the methodology of previous BTN studies2,9,10. Hemolymph and foot tissues were genotyped separately for nuclear microsatellites and EF1α, and for the mitochondrial COI and control region (CR). For EF1α and CR, when multiple alleles were present and could not be resolved by sequencing, molecular cloning was employed. Two kinds of evidence for the presence of BTN were considered: genetic chimerism of cancerous individuals, with the hemolymph and the foot tissues being dominated by different sets of alleles, and the identity of “extra” alleles of different cancerous individuals (see “Introduction” section) (“BTN diagnostics”). At the step of “Phylogenetic analyses”, evolutionary relationships of cancer-associated genotypes were assessed. Firstly, all relevant BTN sequences from the previous studies were considered in order to identify the known cancer lineages, if any, affecting mussels from the SOJ. Secondly, all available M. trossulus COI sequences were examined in order to find out whether the cancer alleles identified in the SOJ mussels had been recorded anywhere before and whether they demonstrate an affinity to particular mitochondrial lineages of the host. Finally, we verified the purebred M. trossulus ancestry of mussels from BTN-infected population by genotyping them by three additional taxonomically diagnostic markers (“Species confirmation”) and identified their sex histologically and/or genetically (“Sex identification”).
Sample collection and preprocessing
Mussels were collected by scuba diving at three localities of the SOJ in July–September 2019: Vladivostok city public beach “Vtoraya Rechka” (43°10′ 02′′ N, 131°58′ 07′′ E, depth 5 m, a natural bottom habitat, sample size N = 39, mean shell size L = 25 mm, sample “R”), “Vostok” Marine Biological Station (42°89′ 35′′ N, 132°73′ 33′′ E, depth 5 m, experimental mussel plantation, N = 20, L = 50 mm, sample “V”) and the Gaydamak Bay (42°52′ 04′′ N, 132°41′ 27′′ E, fouling of a mooring buoy anchored at a depth about 5 m about 50 m from the shore, N = 226, L = 37 mm, sample “J”). “Vostok” station is a nature reserve and the least polluted of the studied localities, while Gaydamak is an industrial harbor heavily polluted by sewage. After sampling, the mussels were transported to the laboratory and stored for 2–4 days alive, each sample in a separate aquarium, before the experiments.
Hemolymph was collected from the posterior adductor with the help of a syringe with a 22-gauge needle. Some aliquots of hemolymph were used immediately for flow cytometry, and some were fixed in 4% PFA for future immunochemistry studies. Some aliquots, as well as pieces of mantle and foot tissues from each specimen, were fixed in 70% ethanol for genetic analyses.
Flow cytometry analysis and the interpretation of the results followed Vassilenko and Baldwin19. Hemocytes stained with 4′-6-diamidino-2-phenylindole (DAPI) were analyzed on a CytoFLEX flow cytometer with CytExpert software (Beckman-Coulter, USA). Plots of side scatter SSC-A versus forward scatter FSC-A were used for visualization of cell groups. Duplets were removed by gating on forward scatter height FSC-H against forward scatter FSC-A. Histograms of fluorescence signal PB450-A were used for determination and gating of cells with different levels of ploidy. At least 10,000 events were evaluated for each sample. Histograms of PB450-A were used to estimate ploidy levels of aneuploid peaks relative to the diploid peak of the same specimen and the rate of aneuploid cells in the sample. Mussels were diagnosed as healthy (“DN-rejected”) if the scatter plot SSC-A vs FSC-A and PB450-A histogram of fluorescence indicated only non-proliferating cells (agranulocytes and granulocytes) with one peak for diploid phase or with admixture of very few (< 5%) proliferating cells (minor peak for tetraploid cells). If a cell population with additional peaks was detected, the individuals were considered as “DN-suggested”.
Hemocytology and immunochemistry
All procedures for cell fixation and staining were described in detail in a previous study41. In brief, the cells were stained with TRITC-labeled phalloidin (Molecular Probes) and DAPI (Vector Laboratories) for visualization of actin cytoskeleton and nucleus. We used primary mouse monoclonal antibodies against anti-α-acetylated tubulin (clone 6-11B-1, Sigma Aldrich and proliferating cell nuclear antigen (PCNA, clone PC10, Abcam) for detecting mitotic spindles and proliferating cells, respectively. These antibodies were previously characterized as labeling dividing cells in bivalves41,42,43,44. Observations and images were made with Zeiss LSM 780 confocal laser scanning microscope. A mussel was considered as “DN-confirmed” if non-adherent hemocytes with a high nucleus-to-cytoplasm ratio and a pleomorphic nucleus were detected.
Total DNA was extracted separately from the hemolymph and the foot tissue using the DNeasy Blood and Tissue Kit (Qiagen, USA) according to the manufacturer’s protocol.
The microsatellite marker Mgµ3, polymorphic in M. trossulus, was amplified according to the protocol in the original study45 and subjected to fragment analysis by capillary electrophoresis. Microsatellite fragment patterns were analyzed in GelQuest (https://www.sequentix.de/gelquest/help/index.html). The attempt to amplify other microsatellite loci (Mgµ5, Mgµ6, Mgµ7) was not successful.
Three DNA fragments—an intron-spanning region of the nuclear EF1α gene, a fragment of the mitochondrial COI and a fragment spanning 16S rRNA and CR—were amplified using primer sequences and PCR cycling conditions as in Metzger et al.2 and Yonemitsu et al.10 and sequenced in both directions by the Sanger method. The primers used for COI amplification target the female mitochondrial genome (F-mtDNA), while primers for 16S and CR potentially amplify both male (M-mtDNA) and F-mtDNA10. Due to the doubly uniparental inheritance (DUI) blue mussel females are homoplasmic for F-mtDNA, which is inherited maternally, while males are heteroplasmic, carrying the F-mtDNA in somatic tissues and the paternally inherited M-mtDNA in gonads46.
Sequencing and fragment analysis were performed on Genetic Analyzer ABI Prism 3500xl at the Centre for Molecular and Cell Technologies of St. Petersburg State University Research Park (https://researchpark.spbu.ru/en/biomed-eng). Sequence chromatograms were visually studied in MEGA X software47.
EF1α PCR products from the hemolymph and the foot tissues of the cancerous and the control mussels were subjected to molecular cloning. CR PCR products were cloned from the hemolymph of the cancerous mussels only. Molecular cloning procedures were subcontracted to Evrogen JSC (Russia). Quick-TA kit (Evrogen JSC) was used for cloning, and the plasmids were transformed into competent E. coli (Evrogen JSC). In all the cases at least 16 colonies were sequenced using M13 primers. Some sequences were detected only in one colony. They were probably artificial mutations generated by PCR and molecular cloning procedures such as polymerase errors and random crossing-over of incomplete PCR extension products of original alleles48,49 and therefore were excluded from the following analyses.
In COI, signals from multiple alleles were resolved by sequencing only. If “piggybacks”, that is, overlapping peaks at some positions, were observed on chromatograms, the major peaks were attributed to the presumable cancer allele in the hemolymph samples and to the presumable host allele in the foot samples.
Sequence chromatograms were analyzed in MEGA X47. Sequences were aligned with MUSCLE algorithm with some manual adjustment.
Nucleotide sequences of CR, COI and EF1α from four cancerous mussels were aligned together with the corresponding sequences from a previous BTN study (data on 11 mussels with confirmed BTN)10 and mitochondrial sequences of the Baltic mussel 62mc1037. The 62mc10 genome was previously shown to be similar to cancerous ones10. Alignments by MUSCLE and maximum likelihood phylogenetic trees were generated using MEGA X47, with 100 bootstrap replicates, treating gaps in the alignment as missing data. The same substitution models as in Yonemitsu et al.10 were used for tree generation. The trees were visualized using iTOL tool50. The analysis of BTN2 CR alleles in Yonemitsu et al.10 revealed that they are recombinant molecules with the insertion of M-mtDNA segment into the F-mtDNA. Therefore we employed the RDP4 package51 to detect possible recombination breakpoints in the cancer-associated CR alleles found in our study (Supplementary Fig. S5).
In the comparative analyses of M. trossulus and BTN COI sequences, we considered the data from this study (four cancerous and 20 healthy mussels), those from previous BTN studies summarized by Yonemitsu et al.10 and all publically available M. trossulus COI data10,36,37,52,53,54,55,56,57. The alignment was created by ClustalW algorithm in MEGA X47. COI haplotype diversity was visualized using the TCS haplotype network58 built within the PopART software59. M. trossulus samples were classified by their geographical origin into four groups (“macroregions”), i.e. the Northwest Pacific, Northeast Pacific, Northwest Atlantic and Northeast Atlantic.
Species confirmation and sex identification
According to a recent survey60, the blue mussel populations in the SOJ are overwhelmingly dominated by M. trossulus, but the presence of a “cryptic” species, M. galloprovincialis and its hybrids with M. trossulus cannot be entirely ruled out. Mussels from the “J” sample (N = 21), including four target mussels with DN, were genotyped for three nuclear markers routinely used for discriminating M. trossulus and M. galloprovincialis61, ME15/1662, ITS63 and MAL-I64, using the primers and protocols in the original articles. The DNA extracted from the hemolymph and from the mantle of each mussel were analyzed in parallel. The mussels were also sexed, at first by a microscopic examination of fresh tissues of the mantle, where the gonads in blue mussels are partly localized. It turned out, however, that most mussels were in post-spawning condition and lacked gametes. Therefore we identified their “mitochondrial” sex by the presence or the absence of M-mtDNA 16S haplotypes, following the approach of Rawson and Hilbish65 and using DNA extracted from the mantle.
Flow cytometry of hemolymph revealed two distinct patterns (Fig. 2). Most of the individuals had one peak of hemocytes, interpreted as diploid (Fig. 2a), or a diploid peak with a small admixture of tetraploids (Fig. 2b). These mussels were diagnosed as healthy. The second pattern was revealed in 10 “J” individuals (4% of “J” sample), which had an additional population of aneuploid cells (Fig. 2c–f). Their ploidy, calculated relatively to the 2n peak, varied among individuals from 3.7 to 5.2 n. The proportion of these cells in the hemolymph of different mussels varied from 12 to 98%. These mussels were classified as “DN-suggested”. We did not reveal any significant signal from proliferating neoplastic cells, which could be expected as a third peak at the right side of the aneuploid peak in the histogram. Two “DN suggested” mussels with a moderate proportion of neoplastic hemocytes, J54 (proportion 44.4%) and J111 (26.4%), and two mussels with a high proportion of neoplastic hemocytes, J161 (91%) and J181 (80%) (Fig. 2c–f), were chosen for further analyses along with the control V1.
Hemocytology and immunochemistry
Hemocytological study revealed striking differences between the control mussels on the one hand and all the four DN-suggested mussels on the other hand. DN-suggested individuals had, in addition to normal adherent hemocytes with a low nucleus-to-cytoplasm ratio, also anomalous round non-adherent hemocytes. They looked like hedgehogs on the slides, the resemblance being due to an altered cytoskeleton with prominent actin “spikes”. Their nuclei were pleomorphic, larger than those of normal hemocytes (Fig. 3). We considered these cells as neoplastic and the mussels they belonged to as DN-confirmed.
PCNA staining revealed few neoplastic hemocytes at the DNA synthesis stage (Supplementary Fig. S1). This observation was in line with the results of flow cytometry, which showed a low proliferating rate of the neoplastic cells.
In the microsatellite analysis the fragment size of the Mgµ3 marker varied in the range of 141–146 bp. In healthy specimens (J2–J17, J38) the size and the representation of the amplified fragments (position and height of the peaks on the electropherograms, Supplementary Fig. S2, see also Fig. 1) from the hemolymph and from the foot samples were the same. In contrast, in all the four DN-confirmed mussels the 146 bp fragment was overrepresented in the hemolymph samples in comparison with the foot samples (Fig. 1, Supplementary Fig. S2). At the same time, this fragment, as well as the 144 bp fragment, characteristic of all the cancerous mussels, was also recorded in some healthy mussels, making the results inconclusive.
In sequenced marker genes, the lengths of the fragments in the final alignment were 447–453 bp for EF1α, 622–624 bp for CR and 630 bp for COI. The cloning results are summarized in Table 1 and Supplementary Table S2. The NCBI GenBank accession numbers are in Supplementary Table S3. Hereafter the alleles identified in our study will be designated by letters if initially recorded in the study of Yonemitsu et al.10, and by numerals if newly found, except in a few cases when we wanted to emphasize the similarity between the alleles (e.g. EF1α-G1, CR-1′, see below). It should be noted, however, that the alignments in Yonemitsu et al.10 were slightly longer than here.
The sequencing and molecular cloning of EF1α PCR products revealed no differences between sequences from the hemolymph and from the foot tissues of the control individuals (Supplementary Table S2 and Fig. 1). In contrast, all EF1α sequencing chromatograms from the hemolymph and the foot samples of DN-confirmed mussels showed a mixed signal. Molecular cloning of these PCR products revealed 2–4 different sequences in the foot samples and 2–6 in the hemolymph samples (Table 1, Fig. 1, Supplementary Fig. S3). Some sequences were common, that is, represented in relatively many colonies, and, with the exception of EF1α-D and EF1α-7, differed by more than one substitution, while others were rare. EF1α-D and EF1α-7 from J161 differed by a single A/T SNP at the 5′ end of the 9 bp-long poly-A repeat (Fig. 1, Supplementary Table S2 and Supplementary Fig. S3). This polymorphism could be artificial. All the mussels had two common sequences, EF1α-G and EF1α-H. They differed by 21 substitutions, which made them the most dissimilar common sequences, and were always more frequent in the hemolymph than in the foot samples. Putatively, EF1α-G and EF1α-H represented a heterozygous cancer genotype. Other common sequences (considering EF1α-D and EF1α-7 to be one and the same sequence) probably represented the diploid host genomes (Table 1). Rare sequences, including EF1α-G1 different from EF1α-G by one substitution (Supplementary Fig. S3), were probably methodological artifacts.
Direct sequencing of COI and CR revealed identical alleles in the hemolymph and in the foot samples of individual control mussels, in homoplasmic condition (J17 and J38, Supplementary Table S2). On the contrary, the chromatograms from analyses of different tissues of mussels with DN looked very different.
No heteroplasmy was observed in the CR chromatograms of cancerous mussels. In foot samples, unique alleles were identified. In the hemolymph samples, two alleles were identified: CR-1 in J54 and J161 and CR-2 in J111 and J181. CR-1 and CR-2 were very different both from each other (31 substitutions, 5.0% difference) and from the other alleles (2.7–6.6%), considering that the differences between all the other alleles were within the range of 0.3–1.5%. Molecular cloning confirmed the results of direct sequencing, but also revealed additional rarer sequences invisible on sequencing chromatograms (Table 1, Fig. 1 and Supplementary Table S2). In the hemolymph of J111 and J181 the same alleles as in foot were found, while in the hemolymph of J161 an allele CR-1′, supported by five clones, was found, differing from the major CR-1 allele by three substitutions (Table 1).
No COI heteroplasmy was observed in the foot samples of cancerous mussels while several positions with overlapping peaks of a very different height were observed on chromatograms of the hemolymph samples (cf. Fig. 1). The heteroplasmy was readily identified as representing presence of the “foot allele” of the same individual in minority (lower peaks) in addition to a dominant hemolymph allele. Two major COI sequences were identified in the hemolymph samples: COI-1 in J54 and J161 and COI-2 in J111 and J181 (Table 1). These alleles differed from each other by 6 substitutions (0.95%) and by 0.60–0.95% from all the other alleles.
Thus, the sequence analyses revealed genetic chimerism of mussels with DN, with the hemolymph and the foot tissues being dominated by different genotypes of both the nucleus and mitochondrion. However, while EF1α genotyping revealed the same cancer genotype in all the diseased mussels, mtDNA genotyping revealed two different cancer genotypes, marked by different combinations of COI and CR alleles, in different mussels. The conclusive evidence that DN in mussels from the SOJ is BTN came from a genetic comparison with cancers from previous studies.
Maximum likelihood trees
A general inspection of phylogenetic trees (Fig. 4) shows that the SOJ mussels are infected with the BTN2 cancer lineage. The EF1α-G and EF1α-H alleles identified in these mussels are previously known BTN2-specific alleles from other Mytilus hosts. For both mtDNA fragments the cancerous alleles clustered together with the major BTN2-specific alleles and the 62mc10 (Fig. 4). The alleles COI-1 and COI-2 differed from the major COI-B BTN2 allele by 6 and 8 substitutions, respectively. CR-1 allele differed from the closest CR-D allele by 16 substitutions, and from the 62mc10 by 11 substitutions. CR-2 differed from the closest CR-C allele by 5 substitutions. The alleles of M. trossulus (i.e. host alleles) from the SOJ were randomly scattered across the M. trossulus clade on the trees (Fig. 4).
An analysis of recombination identified the same breakpoints in CR-1/CR-1′ and CR-D alleles but different breakpoints in CR-2 and CR-C alleles (Supplementary Fig. S5). However, CR-2 and CR-C differed by only two substitutions between the suggested breakpoints. We will therefore adhere to the hypothesis that CR-1 and CR-D, as well as CR-2 and CR-C, represent the same mitochondrial lineages originated through singular recombination events.
In addition to the genetic similarity of BTN2 worldwide, Fig. 4 also illustrates geographic differences within this cancer. In the SOJ there are basically two cancer mtDNA haplotypes, comprising two 1% divergent COI alleles and two very divergent CR alleles (CR-1, CR-2), while elsewhere there are two cancer haplotypes, comprising basically the same COI alleles of the “B group” and two CR alleles (CR-C, CR-D) similar to that in the SOJ. Another difference is that the two cancer haplotypes are apparently homoplasmic in the SOJ and in Europe but heteroplasmic in Argentina (both alleles present in the same cancerous mussels). To remember, individual J161 was heteroplasmic for close CR-1 and CR-1′ alleles. Such “additional” variation which theoretically could be caused by repeat regions in complex CR10 or numts but most probably represents heteroplasmy, occasionally occurs in BTN2 worldwide (Mch-41, Castro-26, Fig. 5). Haplotype network.
Among the COI data sets included in the analysis, that from Vancouver Island, British Columbia54 demonstrated a remarkably strong polymorphism in comparison with other regional sets, including another Northeast Pacific set. Therefore we provide separate networks performed without and with the data of Crego-Prieto et al.54 in Fig. 5 and Supplementary Fig. S4, respectively. The analyses revealed a complex star-like haplotype network familiar from the previous phylogeographic studies34,36,53. The network consisted of several major clades, each with a common core haplotype and many rare haplotypes radiating from it. Some clades were “cosmopolitan” and included samples from both the Atlantic and the Pacific oceans, while others were nearly restricted to the Pacific. The unique BTN1 allele belonged to one of the cosmopolitan clades, which included sequences from all the four macroregions considered but was dominated by samples from the Northeast Pacific. The BTN2 alleles, including that from the SOJ, and the Baltic 62mc10, were attached to another clade. This clade included samples from all the macroregions except the Northeast Pacific (Fig. 5), with one notable exception. A single sequence identical to the cancerous COI-1 from the SOJ was identified in the data from Bamfield locality on Vancouver Island (KF93180554, Supplementary Fig. 7).
Species confirmation and sex identification
Only M. trossulus alleles were recorded in a subsample of mussels (N = 21, including J17, J38, and cancerous J54, J111, J161 and J181) studied by three additional nuclear markers, and the genotypes retrieved from different tissues of the same mussels were always the same. Twelve mussels were identified as “mitochondrial males” by 16S locus, among them J181, and the other mussels, as females.
In this study we showed that Mytilus trossulus mussels from the SOJ, Northwest Pacific, were affected with disseminated neoplasia (DN) and confirmed that it was caused by clonally transmitted cancer (CTC), by demonstrating genetic chimerism of mussels with DN and a striking similarity among their “extra” genotypes. The cancer alleles found in our study did not match those of the BTN1 lineage from M. trossulus populations on the American coast of the Pacific Ocean but matched the alleles of BTN2 lineage, which has been previously diagnosed in M. edulis from Europe and in M. chilensis from Chile and Argentine but not in M. trossulus, from which it is originally derived from. So, we conclude that M. trossulus from the SOJ are infected by BTN2. This finding implies that this species, contrary to the hypothesis of Yonemitsu et al.10, has not evolved resistance to this disease. Below we will first discuss the pathology and epidemiology of BTN2 in mussels from the SOJ and then its genetic properties.
The features of the neoplastic hemocytes in our study—a rounded shape, a large nucleus, a high nucleus-to-cytoplasm ratio and an increased ploidy—agree with the previous descriptions of DN in Mytilus14,22,23. What seems unusual is their low proliferation level. Neoplastic hemocytes of mussels are generally assumed to have a high proliferation activity20. However, a low proliferation rate of neoplastic hemocytes in mussels with DN was reported in two other studies: of BTN (supposedly BTN2) in France22 and of DN66 in the same Argentinean population where BTN2 was recognized later10. A possible explanation is that in case of BTN2 the proliferation site of the neoplastic cells is located not in the hemolymph. This hypothesis is inspired by the study of Burioli et al.22, who observed a high mitotic rate of neoplastic cells in the vesicular connective tissue of BTN-infected mussels.
Our data complement the results of another study of DN in mussels from the SOJ40, where only one individual with DN was found in a histological examination of 40 mollusks from various localities. We only found DN in one of the three populations examined. The DN prevalence in this Gaydamak Bay population (4.0%) was probably underestimated, being based on flow cytometry, which is not very sensitive at the early stages of the disease19,22. Still, our estimate of DN level in the population from the Gaydamak Bay is close to the mean prevalence reported for Mytilus populations worldwide39,67,68,69,70 and much lower than the maximal prevalence of 56% reported for M. trossulus population from British Columbia71.
Noteworthy, the mussels in the Gaydamak Bay were collected from the surface of a mooring buoy in a heavily polluted area, where no mussels were recorded at the sea floor (our observations). Since BTN is presumably transmitted by cancer cells through the water column (see Caza et al.72 for more discussion), we suspect that the mussels fouling the buoy contracted the infection from those that had fouled ships moored to it. We point out that mussel populations on mooring buoys, docks etc. may serve as BTN reservoirs while mussel-fouled ships may be the vectors of the disease.
An association between an increased prevalence of DN in mollusks and a high concentration of pollutants, though often surmised, has never been shown explicitly24. Our samples from other localities than Gaydamak were limited, and we have no reasons to suppose that mussel populations outside harbors in the SOJ are free from the disease. M. trossulus populations in the SOJ and in the Northwest Pacific in general may be a natural reservoir of BTN2, where it is maintained and whence it spreads worldwide.
We recorded four new BTN2 genotypes, in addition to the 11 BTN cancer genotypes reported earlier worldwide (eight of them representing BTN2)2,10. We confirm the conclusions of Yonemitsu et al.10 that BTNs are marked by lineage-specific genotypes at the conservative nuclear EF1α locus and that mitochondrial diversity is observed across BTN2 clones from different individuals as well as within some individuals. This diversity is difficult to interpret at the moment, firstly because of the scarcity of data and secondly because of the possibility of mitochondrial capture from the host and mitochondrial recombination10,33,73.
The two main mitochondrial haplotypes defined as the combinations COI-1 + CR-1 and COI-2 + CR-2, found in homoplasmic condition in our material, were similar but not identical to the two common cancer-associated haplotypes which combine the COI-B alleles with the CR-D and CR-C alleles, respectively, as found by Yonemitsu et al.10 either in heteroplasmic (Argentina) or homoplasmic state (Europe, CR-D allele).
It is also possible that the apparent homoplasmy of the SOJ mussel cancers is spurious. Yonemitsu et al.10 have shown using qPCR that the levels of various haplotypes in heteroplasmic cancer clones may be very different. Since we employed molecular cloning of CR and sequenced a limited numbers of colonies (though more than Yonemitsu et al.10 did to demonstrate heteroplasmy), we might have overlooked rare alleles. Further, if we assume that the cancer clones from Gaydamak are homoplasmic, it follows that the mussels fouling the same mooring buoy were infected with at least two independent clones, which is unlikely, though not impossible.
One novel finding in our study is a remarkable divergence between the two BTN2 haplotypes in the SOJ. Two COI alleles differed from each other and from “B alleles” on average by six substitutions (~ 1%). This salient diversity has probably accumulated after the emergence of BTN2. Most probably, the cancer emerged long before DN was first diagnosed in blue mussels in the 1960s15.
As to the geographical origin of the BTN2 COI diversity, the comparison with a rich collection of M. trossulus COI sequences indicates that it most probably lies outside the Northeast Pacific because cancerous haplotypes represent a common M. trossulus haplogroup widespread in the Atlantic and the Northwest Pacific but virtually absent from the Northeast Pacific populations of this species (see also below). Intriguingly, the unique COI allele of the other cancer lineage, BTN1, so far encountered only in British Columbia10, also belongs to a haplogroup that is much more common in the Atlantic and the Northwest Pacific than in the Northeast Pacific. Hence our analysis did not unambiguously confirm the “endemism” of BTN1 to the NE Pacific (Fig. 5).
At least two of the published M. trossulus sequences considered in our analyses could indeed turn out to be cancer genotypes. One of them is COI KF931805 from British Columbia54, which is identical to the BTN2 allele COI-1. This might mean that BTN2 is cryptically present in British Columbia. If so, DN in mussels from this region could be caused by both BTN1 and BTN2.
Another candidate for a cancerous sequence is KM192133 from the Baltic Sea (genome 62mc10)37, which closely matches BTN2 haplotypes (Fig. 4). Yonemitsu et al.10 considered 62mc10 as a genome of “a normal M. trossulus from the Baltic region”, which is close to the ancestral sequence of BTN2, rather than the genome of the cancer itself. There are, however, several reasons to consider the possibility that 62mc10 might be cancerous. Firstly, M. trossulus from the Baltic Sea themselves generally lack the typical M. trossulus mtDNA. Instead they bear the M. edulis mtDNA, as a consequence of introgressive hybridization between these species74,75. In fact, 62mc10 is the only M. trossulus like mitochondrial sequence revealed in extensive studies of the Baltic mussels37. Secondly, 62mc10 was identified in the mantle (i.e. the gonad) of a female alongside with the standard M. edulis F-mtDNA37. At the same time, 62mc10, as well as BTN2 mtDNA, is a mosaic sequence: F-mtDNA with M-mtDNA CR segments10,37. In mussels, such recombinant mtDNA are usually inherited as standard M-mtDNA (“masculinized” genomes) and so are expected to be found, in a mixture with the F-mtDNA, in gonads of males, not females52,76. The mantle tissues are subject to cancer14, which can explain the heteroplasmy, and DN has indeed been recorded in the Baltic Sea M. trossulus39.
The origin of the two cancerous complex mitochondrial haplotypes—so divergent in their control regions, occurring sometimes together and sometimes apart—remains enigmatic. There is little we can add on this matter to the discussion in Yonemitsu et al.10. BTN2 haplotypes resemble the “masculinized” mitochondrial genomes of mussels. These genomes are common in the Baltic mussels, in which they are M. edulis-derived (with the sole exception of 62mc10), and in the hybrid zone between M. edulis and M. trossulus in Norway, in which they are M. trossulus-derived, but rare elsewhere38,77. Recombination and masculinization in the Baltic and in Norway are thought to be driven by hybridization between M. edulis and M. trossulus37,38. The ubiquity of masculinized genomes in these two regions prompted Yonemitsu et al.10 to suggest that BTN2 originated in one of them. If this hypothesis is true, more extensive genetic surveys would find traces of introgression from M. edulis in the BTN2 nuclear genome. For example, the absolute majority of the Baltic mussels bear M. edulis alleles at the ITS multicopy gene78. The lack of M. edulis ITS alleles in the hemolymph of cancerous mussels from the SOJ in our study is an additional though not conclusive argument against the Baltic origin of BTN2. While the European origin of BTN2 cannot be refuted, we suggest an alternative hypothesis that it emerged in the heart of M. trossulus ancestral range in the Norhwest Pacific.
The similarity between BTN2 and “masculinized” mtDNA might indicate not only the population of the BTN2 origin but also the tissue where it originated and the sex of “patient zero”, the mussel from which BTN2 derive. During embryonic development, paternally inherited mtDNA are maintained in the germline of males79, being the genetic marker of male germ cells. This could mean that cancer cells are male germ cells but not hemocytes by origin. If this is true, the first mussel with BTN2 was a male.
The sequences generated in this study are deposited in the NCBI GenBank. The accession numbers are listed in Supplementary Table 3. Alignment used for tree generation available as Supplementary files.
Murchison, E. P. Clonally transmissible cancers in dogs and Tasmanian devils. Oncogene 27, S19–S30 (2008).
Metzger, M. J. et al. Widespread transmission of independent cancer lineages within multiple bivalve species. Nature 534, 705–709 (2016).
Storfer, A. et al. The devil is in the details: Genomics of transmissible cancers in Tasmanian devils. PLoS Pathog. 14, 1–7 (2018).
Nowinsky, M. A. Zur Frage über die Impfung der krebsigen Geschwülste. Zentralbl Med Wissensch. 14, 790–791 (1876).
Murgia, C., Pritchard, J. K., Kim, S. Y., Fassati, A. & Weiss, R. A. Clonal origin and evolution of a transmissible cancer. Cell 126, 477–487 (2006).
Pearse, A. M. & Swift, K. Allograft theory: transmission of devil facial-tumour disease. Nature 439, 549 (2006).
Siddle, H. V. et al. Transmission of a fatal clonal tumor by biting occurs due to depleted MHC diversity in a threatened carnivorous marsupial. Proc. Natl. Acad. Sci. USA 104, 16221–16226 (2007).
Metzger, M. J. J., Reinisch, C., Sherry, J. & Goff, S. P. P. Horizontal transmission of clonal cancer cells causes leukemia in soft-shell clams. Cell 161, 255–263 (2015).
Riquet, F., Simon, A. & Bierne, N. Weird genotypes? Don’t discard them, transmissible cancer could be an explanation. Evol. Appl. 10, 140–145 (2017).
Yonemitsu, M. A. et al. A single clonal lineage of transmissible cancer identified in two marine mussel species in South America and Europe. Elife 8, 1–21 (2019).
Woods, G. M., Bruce Lyons, A. & Bettiol, S. S. A devil of a transmissible cancer. Trop. Med. Infect. Dis. 5, 1–10 (2020).
Ganguly, B., Das, U. & Das, A. K. Canine transmissible venereal tumour: a review. Vet. Comp. Oncol. 14, 1–12 (2016).
Paynter, A. N., Metzger, M. J., Sessa, J. A. & Siddall, M. E. Evidence of horizontal transmission of the cancer-associated Steamer retrotransposon among ecological cohort bivalve species. Dis. Aquat. Organ. https://doi.org/10.3354/dao03113 (2017).
Barber, B. J. Neoplastic diseases of commercially important marine bivalves. Aquat. Living Resour. 17, 449–466 (2004).
Farley, C. A. Sarcomatoid proliferative disease in a wild population of blue mussels (Mytilus edulis). J. Natl. Cancer Inst. 43, 509–516 (1969).
Sparks, A. K. Synopsis of Invertebrate Pathology Exclusive of Insects (Elsevier, 1985).
Muttray, A. F. & Vassilenko, K. Mollusca: disseminated neoplasia in bivalves and the p53 protein family. Adv. Comp. Immunol. https://doi.org/10.1007/978-3-319-76768-0 (1969).
Bihari, N., Mičić, M., Batel, R. & Zahn, R. K. Flow cytometric detection of DNA cell cycle alterations in hemocytes of mussels (Mytilus galloprovincialis) off the Adriatic coast Croatia. Aquat. Toxicol. 64, 121–129 (2003).
Vassilenko, E. & Baldwin, S. A. Using flow cytometry to detect haemic neoplasia in mussels (Mytilus trossulus) from the Pacific Coast of Southern British Columbia Canada. J. Invertebr. Pathol. 117, 68–72 (2014).
Moore, J. D., Elston, R. A., Drum, A. S. & Wilkinson, M. T. Alternate pathogenesis of systemic neoplasia in the bivalve mollusc Mytilus. J. Invertebr. Pathol. 58, 231–243 (1991).
Benabdelmouna, A., Saunier, A., Ledu, C., Travers, M. A. & Morga, B. Genomic abnormalities affecting mussels (Mytilus edulis-galloprovincialis) in France are related to ongoing neoplastic processes, evidenced by dual flow cytometry and cell monolayer analyses. J. Invertebr. Pathol. 157, 45–52 (2018).
Burioli, E. A. V. et al. Implementation of various approaches to study the prevalence, incidence and progression of disseminated neoplasia in mussel stocks. J. Invertebr. Pathol. 168, 107271 (2019).
Moore, C. A., Beckmann, N. & Patricia Morse, M. Cytoskeletal structure of diseased and normal hemocytes of Mya arenaria. J. Invertebr. Pathol. 60, 141–147 (1992).
Carballal, M. J., Barber, B. J., Iglesias, D. & Villalba, A. Neoplastic diseases of marine bivalves. J. Invertebr. Pathol. https://doi.org/10.1016/j.jip.2015.06.004 (2015).
Odintsova, N. A. Leukemia-like cancer in bivalves. Russ. J. Mar. Biol. 46, 59–67 (2020).
Smolarz, K., Renault, T. & Wołowicz, M. Ultrastructural study of neoplastic cells in Macoma balthica (Bivalvia) from the Gulf of Gdansk (Poland). J. Invertebr. Pathol. 92, 79–84 (2006).
Carella, F. et al. Nuclear morphometry and ploidy of normal and neoplastic haemocytes in mussels. PLoS ONE 12, e0173219 (2017).
Smolowitz, R. M. & Reinisch, C. L. Indirect peroxidase staining using monoclonal antibodies specific for Mya arenaria neoplastic cells. J. Invertebr. Pathol. 48, 139–145 (1986).
Carella, F., Figueras, A., Novoa, B. & De Vico, G. Cytomorphology and PCNA expression pattern in bivalves Mytilus galloprovincialis and Cerastoderma edule with haemic neoplasia. Dis. Aquat. Organ. 105, 81–87 (2013).
McDonald, J. H., Seed, R. & Koehn, R. K. Allozymes and morphometric characters of three species of Mytilus in the Northern and Southern Hemispheres. Mar. Biol. 111, 323–333 (1991).
Larraín, M. A., Zbawicka, M., Araneda, C., Gardner, J. P. A. & Wenne, R. Native and invasive taxa on the Pacific coast of South America: impacts on aquaculture, traceability and biodiversity of blue mussels (Mytilus spp.). Evol. Appl. 11, 298–311 (2018).
Pye, R. J. et al. A second transmissible cancer in Tasmanian devils. Proc. Natl. Acad. Sci. USA 113, 374–379 (2016).
Strakova, A. et al. Mitochondrial genetic diversity, selection and recombination in a canine transmissible cancer. Elife 5, 1–25 (2016).
Rawson, P. D. & Harper, F. M. Colonization of the northwest Atlantic by the blue mussel, Mytilus trossulus postdates the last glacial maximum. Mar. Biol. 156, 1857–1868 (2009).
Wenne, R., Bach, L., Zbawicka, M., Strand, J. & McDonald, J. H. A first report on coexistence and hybridization of Mytilus trossulus and M. edulis mussels in Greenland. Polar Biol. 39, 343–355 (2016).
Laakkonen, H. M., Hardman, M., Strelkov, P. & Väinölä, R. Cycles of trans-Arctic dispersal and vicariance, and diversification of the amphi-boreal marine fauna. J. Evol. Biol. https://doi.org/10.1111/jeb.13674 (2020).
Zbawicka, M., Wenne, R. & Burzyński, A. Mitogenomics of recombinant mitochondrial genomes of Baltic Sea Mytilus mussels. Mol. Genet. Genom. 289, 1275–1287 (2014).
Śmietanka, B. & Burzyński, A. Disruption of doubly uniparental inheritance of mitochondrial DNA associated with hybridization area of European Mytilus edulis and Mytilus trossulus in Norway. Mar. Biol. https://doi.org/10.1007/s00227-017-3235-5 (2017).
Sunila, I. Histopathology of mussels (Mytilus edulis L.) from the Tvarminne area, the Gulf of Finland (Baltic Sea). Ann. Zool. Fennici 24, 55–69 (1987).
Usheva, L. N. & Frolova, L. T. Neoplasia in the connective tissue tumor in the mussel Mytilus trossulus from a polluted region of Nakhodka Bay, the Sea of Japan. Ontogenez 31, 63–70 (2000).
Maiorova, M. A. & Odintsova, N. A. β integrin-like protein-mediated adhesion and its disturbances during cell cultivation of the mussel Mytilus trossulus. Cell Tissue Res. 361, 581–592 (2015).
Marigomez, I., Lekube, X. & Cancio, I. Immunochemical localisation of proliferating cells in mussel digestive gland tissue. Histochem. J. 31, 781–788 (1999).
Maiorova, M. A. & Odintsova, N. A. Proliferative potential of larval cells of the mussel Mytilus trossulus and their capacity to differentiate into myogenic cells in culture. Russ. J. Mar. Biol. 42, 281–285 (2016).
Voronezhskaya, E. E., Nezlin, L. P., Odintsova, N. A., Plummer, J. T. & Croll, R. P. Neuronal development in larval mussel Mytilus trossulus (Mollusca: Bivalvia). Zoomorphology 127, 97–110 (2008).
Presa, P., Pérez, M., Diz, A. P., Perez, M. & Diz, A. P. Polymorphic microsatellite markers for blue mussels (Mytilus spp.). Conserv. Genet. 3, 441–443 (2002).
Zouros, E. Biparental inheritance through uniparental transmission: the doubly uniparental inheritance (DUI) of mitochondrial DNA. Evol. Biol. 40, 1–31 (2013).
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).
Paabo, S., Irwin, M. & Wilson, C. DNA damage promotes jumping between templates during enzymatic amplification. J. Biol. Chem. 265, 4718–4721 (1990).
Bradley, R. D. & Hillis, D. A. Recombinant DNA sequences generated by PCR amplification. Mol. Biol. Evol. 14, 592–593 (1997).
Letunic, I. & Bork, P. Interactive Tree of Life (iTOL) v4: recent updates and new developments. Nucl. Acids Res. 47, 256–259 (2019).
Martin, D. P., Murrell, B., Golden, M., Khoosal, A. & Muhire, B. RDP4: detection and analysis of recombination patterns in virus genomes. Virus Evol. 1, 1–5 (2015).
Breton, S., Burger, G., Stewart, D. T. & Blier, P. U. Comparative analysis of gender-associated complete mitochondrial genomes in marine mussels (Mytilus spp.). Genetics 172, 1107–1119 (2006).
Marko, P. B. et al. The ‘Expansion-contraction’ model of Pleistocene biogeography: rocky shores suffer a sea change?. Mol. Ecol. 19, 146–169 (2010).
Crego-Prieto, V., Juanes, F. & Garcia-Vazquez, E. Aquaculture and the spread of introduced mussel genes in British Columbia. Biol. Invasions https://doi.org/10.1007/s10530-015-0853-z (2015).
Chung, J. M. et al. Molecular phylogenetic study of bivalvia from four countries (China, Japan, Russia and Myanmar) using 3 types of primers. Korean J. Malacol. 35, 137–148 (2019).
Layton, K. K. S., Martel, A. L., Hebert, P. D. N. & Layton, K. K. S. Patterns of DNA barcode variation in Canadian Marine molluscs. PLoS ONE 9, 1–9 (2014).
deWaard, J. R. et al. A reference library for Canadian invertebrates with 1.5 million barcodes, voucher specimens, and DNA samples. Sci. Data 6, 1–12 (2019).
Clement, M., Snell, Q., Walker, P., Posada, D. & Crandall, K. TCS: Estimating Gene Genealogies. Parallel Distrib. Process. Symp. Int. 2, 184 (2002).
Leigh, J. W. & Bryant, D. POPART: full-feature software for haplotype network construction. Methods Ecol. Evol. 6, 1110–1116 (2015).
Kartavtsev, Y. P., Masalkova, N. A. & Katolikova, M. V. Genetic and morphometric variability in settlements of two mussel species (Mytilus ex. Gr. Edulis), Mytilus trossulus and Mytilus galloprovincialis, in the Northwestern Sea of Japan. J. Shellfish Res. 37, 103–119 (2018).
Larraín, M. A., González, P., Pérez, C. & Araneda, C. Comparison between single and multi-locus approaches for specimen identification in Mytilus mussels. Sci. Rep. 9, 1–13 (2019).
Inoue, K., Waite, J. H., Matsuoka, M., Odo, S. & Harayama, S. Interspecific variations in adhesive protein sequences of Mytilus edulis, M. galloprovincialis, and M. trossulus. Biol. Bull. 189, 370–375 (1995).
Heath, D. D., Rawson, P. D. & Hilbish, T. J. PCR-based nuclear markers identify alien blue mussel Mytilus spp. genotypes on the west coast of Canada. Can. J. Fish. Aquat. Sci. 52, 2621–2627 (1995).
Rawson, P. D., Secor, C. L. & Hilbish, T. J. The effects of natural hybridization on the regulation of doubly uniparental mtDNA inheritance in blue mussels (Mytilus spp.). Genetics 144, 241–248 (1996).
Rawson, P. D. & Hilbish, T. J. Distribution of male and female mtDNA lineages in populations of blue mussels, Mytilus trossulus and M. galloprovincialis, along the Pacific coast of North America. Mar. Biol. 124, 245–250 (1995).
Cremonte, F., Vázquez, N. & Silva, M. R. Gonad atrophy caused by disseminated neoplasia in Mytilus chilensis cultured in the Beagle channel, Tierra Del Fuego Province Argentina. J. Shellfish Res. 30, 845–849 (2011).
Ciocan, C. & Sunila, I. Disseminated neoplasia in blue mussels, Mytilus galloprovincialis, from the Black Sea Romania. Mar. Pollut. Bull. 50, 1335–1339 (2005).
Gombač, M., Sitar, R., Pogačnik, M., Arzul, I. & Jenčič, V. Haemocytic neoplasia in Mediterranean mussels (Mytilus galloprovincialis). Mar. Freshw. Behav. Physiol. 46, 135–143 (2013).
Villalba, A., Mourelle, S. G., Carballal, M. J. & López, C. Symbionts and diseases of farmed mussels Mytilus galloprovincialis throughout the culture process in the Rias of Galicia (NW Spain). Dis. Aquat. Organ. 31, 127–139 (1997).
Cremonte, F., Puebla, C., Tillería, J. & Videla, V. Estudio histopatológico del chorito Mytilus chilensis (Mytilidae) y del culengue Gari solida (Psammobiidae) en el sur de Chile. Lat. Am. J. Aquat. Res. 43, 248–254 (2015).
Vassilenko, E. I., Muttray, A. F., Schulte, P. M. & Baldwin, S. A. Variations in p53-like cDNA sequence are correlated with mussel haemic neoplasia: a potential molecular-level tool for biomonitoring. Mutat. Res. Genet. Toxicol. Environ. Mutagen. https://doi.org/10.1016/j.mrgentox.2010.06.001 (2010).
Caza, F., Bernet, E., Veyrier, F. J., Betoulle, S. & St-Pierre, Y. Hemocytes released in seawater act as Trojan horses for spreading of bacterial infections in mussels. Sci. Rep. 10, 1–12 (2020).
Rebbeck, C. A., Leroi, A. M. & Burt, A. Mitochondrial capture by a transmissible cancer. Science (80-) 331, 303 (2011).
Rawson, P. D. & Hilbish, T. J. Asymmetric introgression of mitochondrial DNA among European populations of Blue Mussels (Mytilus spp.). Evolution (N. Y.) 52, 100–108 (1998).
Kijewski, A., Zbawicka, M., Väinölä, R. & Wenne, T. K. Introgression and mitochondrial DNA heteroplasmy in the Baltic populations of mussels Mytilus trossulus and M. edulis. Mar. Biol. https://doi.org/10.1007/s00227-006-0316-2 (2006).
Burzyński, A., Zbawicka, M., Skibinski, D. O. F. & Wenne, R. Evidence for recombination of mtDNA in the marine mussel Mytilus trossulus from the Baltic. Mol. Biol. Evol. 20, 388–392 (2003).
Burzynski, A., Zbawicka, M., Skibinski, D. O. F. & Wenne, R. Doubly uniparental inheritance is associated with high polymorphism for rearranged and recombinant control region haplotypes in Baltic Mytilus trossulus. Genetics 174, 1081–1094 (2006).
Stuckas, H., Stoof, K., Quesada, H. & Tiedemann, R. Evolutionary implications of discordant clines across the Baltic Mytilus hybrid zone (Mytilus edulis and Mytilus trossulus). Heredity (Edinb). 103, 146–156 (2009).
Cao, L., Kenchington, E. & Zouros, E. Differential segregation patterns of sperm mitochondria in embryos of the Blue Mussel (Mytilus edulis). Genetics https://doi.org/10.1534/genetics.166.2.883 (2004).
We would like to thank Natalia Lentsman for English language editing of the manuscript, Marina Katolikova for making cell drawings for Figure 1, Anna Romanovich and Alexey Masharskiy from the Centre for Molecular and Cell Technologies for technical help. This study was supported by Russian Science Foundation, Grant Number 19-74-20024.
The authors declare no competing interests.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
About this article
Cite this article
Skazina, M., Odintsova, N., Maiorova, M. et al. First description of a widespread Mytilus trossulus-derived bivalve transmissible cancer lineage in M. trossulus itself. Sci Rep 11, 5809 (2021). https://doi.org/10.1038/s41598-021-85098-5
Nature Ecology & Evolution (2022)