Increased Inter-Colony Fusion Rates Are Associated with Reduced COI Haplotype Diversity in an Invasive Colonial Ascidian Didemnum vexillum

Increased Inter-Colony Fusion Rates Are Associated with Reduced COI Haplotype Diversity in an Invasive Colonial Ascidian Didemnum vexillum

  • Kirsty F. Smith, 
  • Lauren Stefaniak, 
  • Yasunori Saito, 
  • Chrissen E. C. Gemmill, 
  • S. Craig Cary, 
  • Andrew E. Fidler
  • Published: January 31, 2012
  • DOI: 10.1371/journal.pone.0030473


Considerable progress in our understanding of the population genetic changes associated with biological invasions has been made over the past decade. Using selectively neutral loci, it has been established that reductions in genetic diversity, reflecting founder effects, have occurred during the establishment of some invasive populations. However, some colonial organisms may actually gain an ecological advantage from reduced genetic diversity because of the associated reduction in inter-colony conflict. Here we report population genetic analyses, along with colony fusion experiments, for a highly invasive colonial ascidian, Didemnum vexillum. Analyses based on mitochondrial cytochrome oxidase I (COI) partial coding sequences revealed two distinct D. vexillum clades. One COI clade appears to be restricted to the probable native region (i.e., north-west Pacific Ocean), while the other clade is present in widely dispersed temperate coastal waters around the world. This clade structure was supported by 18S ribosomal DNA (rDNA) sequence data, which revealed a one base-pair difference between the two clades. Recently established populations of D. vexillum in New Zealand displayed greatly reduced COI genetic diversity when compared with D. vexillum in Japan. In association with this reduction in genetic diversity was a significantly higher inter-colony fusion rate between randomly paired New Zealand D. vexillum colonies (80%, standard deviation ±18%) when compared with colonies found in Japan (27%, standard deviation ±15%). The results of this study add to growing evidence that for colonial organisms reductions in population level genetic diversity may alter colony interaction dynamics and enhance the invasive potential of newly colonizing species.


Human mediated transfer of species into regions beyond their native range, and the resulting ecosystem perturbations, are major contributors to currently accelerating rates of indigenous biodiversity loss and species extinction [1][3]. In recent years, considerable progress has been made in describing terrestrial and aquatic bioinvasions in terms of the physical mechanisms of propagule transport, phylogenetic relationships, and population genetics [4][6]. Population genetic theory predicts that the small founder populations typical of invasive species, at least in the initial colonization stages, contain an unrepresentative portion of the total genetic variation present in the source population [7], [8] and that further stochastic losses of allelic diversity (i.e. genetic drift) are anticipated in such small populations [4], [7], [9].

Such non-adaptive changes in the genetics of newly colonizing species are expected to have both genotypic and phenotypic consequences, possibly including deleterious inbreeding depression [10], [11]. In addition, a colonizing species is exposed to novel selection pressures in its new environment with its extant genetic diversity strongly influencing its capacity to adaptively evolve in response to these selective pressures [4], [10], [12]. Despite these theoretical predictions, many introduced species with associated genetic bottlenecks have successfully established in new environments and have often out-competed locally-adapted native species [13][15]. Furthermore, reduced genetic diversity in invasive populations is not as common as initially expected; with a recent review concluding only 37% of studies on aquatic invasions reported evidence of significant loss of genetic diversity in the introduced populations [9]. In some cases invasive populations actually appear to have increased genetic diversity in their new environment which has been attributed to admixture of lineages from multiple native populations with differing genetic profiles [16][18].

Biological explanations for the invasive success of particular species can be elusive and general ecological parameters such as release from predation [19], reduced competition [20], or naïve prey in the new environment [21] are often cited as primary causes of invasion success. More recently, progress has been made in identifying specific phenotypic traits that may confer increased invasion success for particular taxa [22][26]. A useful approach to identifying phenotypic traits relevant to invasion success is to compare and contrast biological characteristics of a species in both native and non-native regions [27]. Taking this strategy, in this study we compared both the population genetics and the colony fusion biology of a highly invasive colonial ascidian, Didemnum vexillum, within both its probable native region (Japan) and a recently established, non-native region (New Zealand).

Genetic loci that strongly influence the structure and functioning of biological colonies have been characterized to the molecular level from a diverse range of phyla: Arthropoda [28], Mycetozoa [29], and Chordata [30]. In these examples, a small number of highly polymorphic loci have been described that have profound effects on inter-colony interactions [28][30]. In the context of invasion biology, a potential consequence of such polymorphic genetically based recognition systems is that reduced genetic diversity may actually enhance invasiveness, at least in the short-term, by reducing intra-specific conflict and increasing mean colony size. A well-documented example of such a mechanism is the highly invasive Argentine ant (Linepithema humile) which displays both reduced genetic diversity and reduced inter-colony aggression in non-native regions [26], [31], [32]. In newly introduced populations of Argentine ant founder effects reduce both genetic diversity and intra-specific aggression, enabling the formation of the very large colonies typical of this invasive species [26], [33].

Taxonomically diverse groups of colonial ascidians have been shown to have allorecognition mechanisms that distinguish closely related colonies from unrelated colonies [34][39]. Adjacent, genetically similar colonies are able to fuse to form a single chimeric colony, while genetically dissimilar colonies will not fuse. For the well-studied colonial botryllid ascidian, Botryllus schlosseri, fusion to produce a chimeric colony is a well-described and complex process involving both the tunic and the vascular system that connects the individual zooids that comprise the colony [34][39]. In contrast, the colony fusion process of didemnid ascidians, which lack a common vascular system, is poorly understood [40]. Whatever the details of the fusion process, the resulting chimeric colonies are expected to possess greater genetic variability and possibly display an associated wider range of physiological tolerances [41]. In B. schlosseri a single highly polymorphic locus has been shown to strongly influence colony allorecognition [39], [42], [43]. In such systems, significant reductions in allelic diversity, specifically at allorecognition locus/loci, may have a profound effect on the probability of two randomly-selected colonies in a population being able to fuse, which in turn may influence typical colony sizes and structure [39], [44]. This hypothesis has been previously proposed to explain why some colonial ascidians are such successful invaders [45]. Colonial ascidians appear to be a promising taxonomic group for investigating mechanisms that link population genetics to phenotypic differences in invasive populations.

Over the past decade, morphologically similar colonies of an ascidian, Didemnum sp., from diverse geographical temperate regions have been reported: New Zealand [46], [47], European Atlantic coast [48][50] and the west and east coasts of North America [51]. These various populations were initially designated as five different, and previously described, Didemnum species along with two entirely new species designations for New Zealand (D. vexillum Kott, 2002) and New Hampshire (D. vestum Kott, 2004) [49]. However, subsequent morphological [49] and molecular comparisons [52] concluded that all specimens belonged to a single species: Didemnum vexillum Kott, 2002 [49], [52]. These authors suggested that the native range of D. vexillum was likely to be in the northwest Pacific [49], [52]. In New Zealand, and some other regions in which D. vexillum is considered non-native (e.g. the east coast of North America), D. vexillum often forms very large colonies that may smother other marine invertebrates including commercially valuable aquaculture species [53]. For example, on Georges Bank, east of Cape Cod, Massachusetts, D. vexillum colonies now extend over very large areas - in 2005 estimated as >230 km2 [54].

Didemnum vexillum was first reported in New Zealand in 2001 within two adjacent harbours on the North Island, Tauranga and Whangamata [46]. Later that same year, D. vexillum was identified in the Marlborough Sounds (South Island), initially on a single barge that had earlier been moved from Tauranga harbour [55]. Current evidence strongly suggests that D. vexillum is not native to New Zealand including; a well-defined history of spread, the strong correlation between the distribution of D. vexillum in New Zealand and the infested barge, and that D. vexillum arguably meets all ten of the accepted criteria for designating a species as non-native [53], [56]. Given the tendency of D. vexillum in New Zealand to form large, biofouling colonies [53], we hypothesized that the colonization of New Zealand by D. vexillum was associated with a significant reduction in its genetic diversity and in consequence New Zealand populations may exhibit increased rates of inter-colony fusion. To test this hypothesis, we examined genetic diversity within the D. vexillum mitochondrial cytochrome oxidase I (COI) coding region, comparing samples collected from New Zealand with those from Japan. In parallel we assessed the frequencies with which randomly selected D. vexillum colonies fused in experimental cut surface assays, comparing populations in New Zealand and Japan.


Didemnum vexillum COI haplotypes in New Zealand and Japan

Tissue sample from 98 colonies morphologically identified as being D. vexillum were obtained: Japan, four locations, n = 37 colonies; New Zealand, five locations, n = 61 colonies (Figure S1, Table S1). Mitochondrial COI partial coding sequences (586 bp) were amplified from all 98 specimens. When combined with the previously reported D. vexillum COI sequence dataset [52] (n = 71) the resulting 169 COI sequences grouped into 16 haplotypes, denoted H2–H17. Of the 13 COI haplotypes observed in this study (haplotypes H2, H3, H5, H6, H9–H17; corresponding source locations and GenBank accession numbers listed in the supplementary materials Table S1), seven (haplotypes H11–H17) were not previously reported [52] (Figure 1). All sequence differences between the 13 COI haplotypes were synonymous.

Figure 1. Bayesian phylogenetic analysis of 16 Didemnum vexillum cytochrome oxidase I (COI) haplotypes.

Numbers on nodes denote posterior probability values. GenBank accession numbers of the COI haplotypes are shown. Asterisks indicate seven COI haplotypes (H11–H17) not previously reported by Stefaniak et al. (2009) [52]. COI sequences from Didemnum psammatode (EU742661, JN624758), D. albidum (EU419432, EU419456) and Didemnum sp. B (EU419407, EU419408) were used as outgroups.


Phylogenetic analyses of Didemnum vexillum COI haplotypes

Bayesian phylogenetic analysis of the 16 D. vexillum COI haplotypes revealed two well supported distinct clades, denoted A and B, each supported by posterior probability values of 1.0 (Figure 1). The clear separation of these two COI clades was also apparent in a statistical parsimony network (Figure 2) with 17 hypothetical mutational steps separating the basal nodes of the two clades (Figure 2). Clade A (haplotypes H2–H8) included sequences from five broad sampling regions: New Zealand (NZ), Japan, West Coast North America (WCNA), East Coast North America (ECNA) and Europe (Figure 2). In contrast, the Clade B haplotypes (i.e. H9–H17) were exclusively amplified from the Japanese samples (Table S1, Figure 2).

Figure 2. Statistical parsimony network of 16 Didemnum vexillum cytochrome oxidase I (COI) haplotypes.

Areas of circles are proportional to the frequency of each haplotype in the dataset and differing shading indicates five different geographic regions as indicated. Small black circles on the branches indicate hypothetical intermediate haplotypes that were not observed.


The percentages of polymorphic sites within clades A and B were 1.9% and 2.6%, respectively, while the percentage polymorphic sites within the combined COI sequence dataset was 6.8%. Divergence between clades A and B, as estimated by p-distance, is 0.040 while the number of net nucleotide substitutions per site (Da) between clades A and B is 0.032.

To investigate if the D. vexillum COI sequence based clade structure was reflected in the nuclear genome, 18S rDNA sequences were amplified from DNA preparations corresponding to the thirteen COI haplotypes found in this study (i.e. haplotypes H2, H3, H5, H6, H9–H17). All 18S ribosomal DNA (rDNA) sequences amplified were identical except at position 705; the 18S rDNA sequences amplified from clade A genomic DNA (COI haplotypes H2, H3, H5 and H6) were A705 while the clade B haplotypes (i.e. H9–H17) were G705 (coordinates of GenBank accession number JF738070).

Population genetic analyses

For population genetic analyses, the D. vexillum COI sequences from both this work and Stefaniak et al. (2009) [52] (n = 169 in total) were grouped into five distinct geographic regions: NZ (n = 67), Japan (n = 50), WCNA (n = 15), ECNA (n = 27) and Europe (n = 10) (Table 1). To allow for the possibility that the COI sequences of clades A and clade B are derived from two cryptic sibling species, population genetic analyses were carried out using two datasets: the first consisted exclusively of clade A COI sequences (i.e. n = 144 sequences, haplotypes H2–H8) while the second dataset consisted of both the clade A and B sequences combined (i.e. n = 169 sequences, haplotypes H2–H17) (Table 1).

Table 1. Didemnum vexillum cytochrome oxidase I (COI) sequence diversity measures from five geographic regions.


H3 was the only COI haplotype found in all five geographical regions and appears to be the most common world wide (Figure 2). In this study, only two clade A COI haplotypes, H3 and H5, were found within the 61 NZ samples examined (Figure 2, Table 1). Despite extensive sampling from the Marlborough Sounds, NZ (n = 44), we did not recover the H4 haplotype that had previously been reported from the barge that is believed to have transported D. vexillum to the Marlborough Sounds [52]. The paucity of COI haplotypes in NZ (n = 3 haplotypes) is reflected in lower haplotype and nucleotide diversity values when compared with the four other geographical regions (Table 1). ECNA, Europe, and WCNA follow NZ in having low levels of COI haplotype diversity when compared with Japan (Table 1). Of the fifteen COI haplotypes found in Japan, eleven are apparent private haplotypes (H7, H8, H9–H17) with nine of these private haplotypes (H9–H17) placed in clade B (Figure 2, Table 1). No other geographic region had private haplotypes (Table 1). When both clade A and B haplotypes were included in the analysis, Japan had the highest levels of haplotype richness, nucleotide and haplotype diversity (Table 1). In contrast, when the data-set was restricted to the clade A haplotypes, Japan had similar haplotype and nucleotide diversity to WCNA and Europe but haplotype richness was still much higher in Japan (Table 1). ECNA resembles NZ in having very low levels of COI haplotype richness and nucleotide and haplotype diversity (Table 1).

Cut surface assays (CSA) to determine D. vexillum inter-colony fusion compatibility

Four independent CSA experiments were conducted in New Zealand between February and April 2009 (i.e. austral summer/autumn) with an average of eleven CSA pairings (range 21–3), excluding positive controls, for each experiment (Table S2A, Table 2). Positive controls consisted of autogenic parings of samples from the same colony and all positive controls resulted in fusions (Table S2). In New Zealand an average of 80% (standard deviation ±18, range 60–100%) of the CSA pairings resulted in inter-colony fusions (Table 2). Three independent CSA experiments were conducted in Japan in July 2010 with ten pairings for each experiment (Table S2B, Table 2) and an average inter-colony CSA fusion rate of 27% (standard deviation ±15%, range 10–40%, Table 2). CSA determined fusion rates in the New Zealand experiments were significantly higher than in Japan (z = 4.53, P = 0.00). There was no significant difference between fusion rates for any experiments within either NZ or Japan. Amplified COI sequences established that all the colonies used in the CSA fusion experiments were from D. vexillum clade A (NZ: haplotypes H3 or H5; Japan: haplotypes H2 or H5; Table S2).

Table 2. Summary of results of cut surface assays (CSA) of Didemnum vexillum carried out in New Zealand and Japan.



Didemnum vexillum COI haplotype diversity within New Zealand is significantly less than within D. vexillum's putative native region in Japan. The New Zealand D. vexillum populations sampled contained as few as three COI haplotypes. These data suggest an interpretation that D. vexillum experienced a significant reduction in genetic diversity when colonizing New Zealand, presumably due to a founder effect. Other putatively introduced populations (i.e., Europe, ECNA, WCNA) also display reduced diversity when compared to Japan, although sample sizes from these regions are small. Reduced genetic diversity is a common, but by no means universal, feature of invasive populations [9]. The genetic diversity of non-native D. vexillum populations will increase with time as further colonization events augment existing genetic variation, although this may not be always be the case [57]. Mitochondrial sequences, being haploid and almost exclusively maternally inherited, are more sensitive to founder events than bi-parentally inherited, diploid nuclear genes [58]. However, the reductions in COI genetic diversity detected in the New Zealand D. vexillum clade A population are potentially associated with reductions in allelic diversity at nuclear loci [59].

Phylogenetic analyses of the sixteen D. vexillum COI haplotypes revealed a well-supported monophyletic D. vexillum species grouping, composed of two distinct well-supported clades, termed A and B. Clade A included haplotypes from all five widely-separated geographical regions defined in this study while clade B was composed of haplotypes found solely in Japan. A previously published COI based D. vexillum phylogeny [52] is consistent with this conclusion, although as only two clade B haplotypes (H9 and H10) were present in this dataset, the clade structure was not so obvious [52]. The high levels of intraspecific genetic variation that are characteristic of ascidian genomes prevent any confident assessment of whether or not D. vexillum clades A and B correspond to cryptic, sibling species or to intra-specific subtypes [60]. A number of recent studies using molecular techniques have concluded that some ascidian species groupings, originally erected on the basis of morphology, actually contain distinct sub-clades [61][65]. The levels of COI sequence variation between, and within, D. vexillum clades A and B, as estimated by percentage of polymorphic sites, are at the lower end of comparable values reported for other ascidian species (e.g., [62], [63], [66], [67]). Furthermore, the level of D. vexillum sequence divergence between COI clades A and B is well below the comparable divergence values for two cryptic species now recognised within the Ciona intestinalis grouping [68], [69]. Additionally, clade B D. vexillum colonies that were examined in a previous global distribution study were deemed morphologically identical to clade A colonies with respect to all characters studied [49]. Both the COI sequence data and the morphological evidence support an interpretation that D. vexillum clades A and B are best regarded, at least for the present, as intra-species variants rather than cryptic species. An apparent lack of inter-clade introgression of two D. vexillum 18S rDNA alleles supports clades A and B being distinct species. However, this interpretation is tentative and needs to be supported by looking at additional, independently segregating, nuclear haplotypes from D. vexillum clade A and B populations occurring in sympatry in Japan. For the present, the most parsimonious conclusion is that D. vexillum COI clades A and B are within the same species grouping and further study is required to resolve this matter.

The lack of an adequate ascidian fossil record prevents calibration of ascidian COI sequence divergence against geological time [69]. However, using the values 1.6–2.6% divergence/million years derived from other marine invertebrate taxa [69] would place divergence of the D. vexillum A and B COI clade lineages at 1.5–2.5 million years ago. Furthermore, as several studies have suggested a faster rate of molecular evolution for tunicates than many other organisms, these times may be over-estimates [70][73]. It appears likely that D. vexillum COI clade A and B lineages diverged within the Pleistocene epoch (2.6 million to 12 000 years BP). Repeated Pleistocene glaciations profoundly affected the oceans around the present day Japanese archipelago [74]. We speculate that clade A and B lineage separation may have occurred in association with such climatic changes – perhaps due to a period of a restricted gene flow between populations in dispersed refugia. It is noteworthy that, from the samples collected to date, D. vexillum clade B appears to be restricted to Japan.

While the fusion biology and associated colony allorecognition genetics of the colonial ascidian B. schlosseri (fam. Styelidae) has been extensively studied [30], [42] little comparable work has been reported for colonial ascidians from the family Didemnidae. Mukai and Watanabe (1974) [34] found evidence of colony allorecognition specificity in Didemnum moseleyi (fam. Didemnidae) whereas Bishop and Sommerfeldt (1999) [38] reported an absence of allorecognition discrimination during colony fusion in Diplosoma listerianum (fam. Didemnidae). Rates of chimeric colonies in natural populations of D. listerianum were also found to be extremely common [75], [76]. In this study we showed that D. vexillum possesses some form of colony recognition mechanism – with autogeneic assays always fusing and some inter-colony fusions resulting in non-fusion reactions. New Zealand populations of D. vexillum clade A displayed higher rates of fusion between paired, randomly-selected colonies than was found in Japan. An average of 80% (standard deviation ±18%) of the New Zealand inter-colony CSAs resulted in fusions compared with a value of 27% (standard deviation ±15%) for Japan. Note that in Japan the D. vexillum colonies were all from clade A and were collected from within a small bay (i.e. Shizugawa Bay) – a sampling strategy which would bias the sampling of related colonies and thereby inflate the CSA fusion rates. These CSA findings are consistent with a model in which reduction of the allelic diversity at D. vexillum's putative allorecognition loci enhances the probability that two randomly selected D. vexillum colonies in recently established populations will be genetically similar enough to fuse.

A major challenge facing invasion biology is the description of biological features that may help predict the chances of invasion success and the delineation of the selective advantage(s) such features provide in novel environments [77]. For colonial organisms, an increased rate of inter-colony fusion might be advantageous as such fusions could result in larger, more genetically diverse and, potentially, more adaptable and competitive colonies [41], [78]. Although there may also be evolutionary costs arising from intra-colony somatic cell competition and germ cell parasitism [35]. In this work, we have shown that reduced genetic diversity at a mitochondrial locus in an introduced population of D. vexillum is correlated with increased rates of fusion between colonies. Such an enhanced tendency towards forming large chimeric colonies might explain the extreme propensity for biofouling that D. vexillum displays outside its putative native range [54], [55]. However, caution is warranted when generalizing the fusions results obtained in this study and it would be illuminating to carry out similar experiments in other invasive populations of D. vexillum. In addition, work investigating the frequency of chimeric colonies in both the New Zealand and Japanese D. vexillum populations is currently underway. The results of the combined population molecular genetic and phenotype-level study reported here suggest a model by which reductions in genetic diversity may enhance the invasiveness and biofouling propensity of D. vexillum. This model also suggests that a potential biocontrol method for D. vexillum outside its native range could be the introduction of additional genetic diversity into the invasive populations. Such introductions of additional genetic diversity would not remove D. vexillum from non-native regions, an undertaking now widely accepted as impossible, but may attenuate D. vexillum's propensity of biofouling that negatively impacts on aquaculture.

Materials and Methods

Ethics statement

No specific permits were required for the described field studies. No locations were privately-owned or protected in any way and the studies did not involve endangered or protected species.

Tissue sampling for population genetics

Tissue samples were taken from colonies morphologically identified as D. vexillum in New Zealand (five locations: Whangamata, Marlborough Sounds, Port Nelson, Wellington Habour, and Lyttelton Harbour) and Japan (four locations: Izu Peninsula, Sagami Bay, Ise Bay, and Shizugawa Bay) between April 2008 and July 2009 (Figure S1, Table S1). Samples were collected from colonies ≥2 m distance apart to minimize the chances of pseudo-replication of sampling from clonally related colonies. Tissue samples (ca. 100–500 mg) were preserved in approx. 2.0 ml of 96% (v/v) ethanol and stored at −20°C.

Amplification of mitochondrial cytochrome oxidase I and 18S ribosomal gene sequences

Tissue samples (ca. 50 mg) were macerated using a sterile scalpel blade. Total genomic DNA was extracted using i-genomic CTB DNA extraction mini kits (animal tissue protocol; Intron, Gyeonggi-do, South Korea). An approximately 600 bp section of the COI gene was amplified using tunicate primers (Tun_forward and Tun_reverse2) [52]. The polymerase chain reaction (PCR) amplifications were carried out in 50 µl reaction volumes containing; 25 µl of i-Taq 2× PCR master mix (Intron, Gyeonggi-do, Korea), 0.4 µM of both forward and reverse primers and 1.0 µl of template containing ca. 50–150 ng of DNA. Thermocycling conditions consisted of an initial denaturing step of 95°C, 4 min, followed by 40 cycles of 94°C, 1 min; 39°C, 1 min; 72°C, 90 seconds; with a final extension step of 72°C, 10 min. If any COI haplotype sequences were found only once, the samples were re-analysed to ensure the observed differences were not due to sequencing error or replication errors during the PCR. An approximately 900 bp section of the 18S rDNA gene was amplified as two overlapping fragments using the PCR primer pairs F16 with R497 and F476 with R917 [79]. PCR mixes were made up as described above with thermocycling conditions of initial denaturing step of 94°C, 2 minutes, followed by 30 cycles of 94°C, 30 seconds; 56°C, 30 seconds, 72°C, 30 seconds; with a final extension step of 72°C, 10 minutes. Amplification products were purified using AxyPrep PCR cleanup kits (Axygen, California, USA) and sequenced in both directions, using the PCR primers, by an external contractor (Waikato University DNA Sequencing Facility, Hamilton, New Zealand). Sequence chromatograms were examined visually and any base-calling errors corrected manually using the BioEdit Sequence Alignment Editor [80]. Both forward and reverse sequences were aligned and any apparent conflicts resolved by manual inspection. For subsequent analyses the COI and 18S sequence data matrices were truncated to 586 bp and 861 bp respectively.

Phylogenetic analyses

The initial data for phylogenetic analyses consisted of the 98 new COI sequences generated as part of this study and 71 previously published sequences [52] (GenBank accession numbers EU419401–EU419406, EU419409–EU419431, EU419433–EU419455, EU419457–EU419459, and EU742662–EU742677). Identical sequences were collapsed into single haplotypes to generate a total of 16 haplotypes. COI sequences from Didemnum psammatode (EU742661, JN624758), D. albidum (EU419432, EU419456) and Didemnum sp. B (EU419407, EU419408) were used as outgroups. Bayesian phylogenetic analyses were performed using MrBayes 3.1.2 [81]. The generalized time reversible model with a proportion of invariable sites and a gamma shaped distribution of rates across sites (GTR+I+gamma) was selected using MrModeltest v 2.2 [82]. The Bayesian analysis was carried out in two simultaneous runs for 5×106 generations, with four chains each and trees were sampled every 100 generations. Of the 5×104 trees sampled the latter 4.9×103, were used to construct a 50% majority-rule consensus tree.

Pairwise distances (the proportion of nucleotide sites that differ between two sequences) and average p-distances were calculated using MEGA 4.0 [83]. The number of net nucleotide substitutions per site (Da) was calculated in DnaSP 5.0 [84].

Population genetic analyses

Mitochondrial COI sequences were first grouped into five broad geographical areas; New Zealand (NZ), Japan, West Coast North America (WCNA), East Coast North America (ECNA) and Europe. For each geographical region four measures of genetic diversity were calculated using ARLEQUIN 3.01 [85]: (i) total COI haplotype numbers, (ii) numbers of private COI haplotypes, (iii) nucleotide diversity, and (iv) haplotype diversity. Haplotype richness was calculated using FSTAT v2.9.3.2 [86]. Using the program TCS 1.21 [87] a 95% statistical parsimony cladogram network of the 16 haplotypes was built.

Cut surface assay (CSA) of inter-colony fusion

To assess the rates of inter-colony fusion within populations of D. vexillum, cut surface assays (CSA) [43] were performed between colonies collected from New Zealand (Marlborough Sounds) and Japan (Shizugawa Bay) (Figure S1, Table S2). Colonies for fusion assays were collected ≥5 m distance apart to minimize the chances of selecting clonally related colonies. Using a scalpel blade, small pieces (ca. 20 mm×20 mm) were cut from two colonies and attached with cotton thread to a Perspex plate (150 mm×150 mm×5 mm) with the cut edges touching. CSA were set up for all collected colony combinations for each experiment. Plates were hung vertically from floating platforms into seawater in sheltered locations at a depth of 2 m. Colonies were left to grow for 3–4 days and then examined for fusion between the tissue samples from different colonies. Autogeneic assays, using two pieces of tissue from the same colony, were used as positive controls. CSA were recorded as fused if the two paired colony fragments could not be pulled apart after three to four days of growth. Although some CSA pairs initially appeared to fuse, the tissue at the fusion zone subsequently decayed and such transient fusions were recorded as non-fusions. Fusion percentages obtained from CSA experiments within NZ, within Japan and between NZ and Japan were compared using two-sided z-tests. COI sequences from all the colonies used in the CSAs were obtained to confirm their taxonomic identity as D. vexillum.

Supporting Information

Figure S1.

Didemnum vexillum colony collection sites for DNA sampling and/or cut surface assays (CSA) in New Zealand (A) and Japan (B). (A) New Zealand sites: Marlborough Sounds (a, Ruakaka Bay; b, Hitaua Bay; c, Onahau Bay; d, Homeward Bay; e, Grant Bay; f, West Beatrix Bay; g, South East Bay; h, Yncyca Bay; I, Fairy Bay; j, Four Fathom Bay; k, Picton; l, Kenepuru Sound); Port Nelson; Wellington Harbour; Port Lyttelton; Whangamata. (B) Japan sites: Shizugawa Bay; Misaki Bay; Izu Peninsula; Ise Bay. Maps are not to scale.



Table S1.

Source and sequence details, including GenBank accession numbers, of the Didemnum vexillum cytochrome oxidase I (COI) sequences from this study.



Table S2.

Results of cut surface assays (CSA) of Didemnum vexillum colonies from New Zealand (A) and Japan (B). Collection sites are indicated with the bracketed letters corresponding to locations in Figure S1. Diagonal boxes show autogenic (i.e. positive control) fusions with the colony's COI haplotype, blank boxes below the diagonal indicate inter-colony pairings that resulted in fusion, boxes with a ‘×’ indicate inter-colony pairings that did not result in fusion.




The authors would like to thank staff at Shimoda Marine Research Center (University of Tsukuba), the Shizugawa Nature Center, Misaki Marine Biological Station (University of Tokyo), Sugashima Marine Biological Laboratory (Nagoya University), and the Asamushi Research Center for Marine Biology (Tohoku University) for assistance with sample collection in Japan. KFS would especially like to thank staff at Shimoda Marine Research Center and the Shizugawa Nature Center for hosting her visits to Japan. The authors would like to thank Aaron Pannell (Marlborough Mussel Company), Brian Coffey (Brian T. Coffey and Associates Limited), Dr. Barrie Forrest and Lauren Fletcher (Cawthron Institute), and Lucie Bizzozero (National Institute of Applied Sciences, Lyon) for assistance with sample collection in New Zealand. Comments from Dr. Phil Lester (Victoria University of Wellington, NZ) and two anonymous reviewers greatly improved earlier drafts of the manuscript.

Author Contributions

Conceived and designed the experiments: KFS AEF. Performed the experiments: KFS AEF YS. Analyzed the data: KSF AEF. Contributed reagents/materials/analysis tools: KFS AEF LS. Wrote the paper: KFS AEF CECG SCC.


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