Myctophids are among the most abundant mesopelagic teleost fishes worldwide. They are dominant in the Southern Ocean, an extreme environment where they are important both as consumers of zooplankton as well as food items for larger predators. Various studies have investigated myctophids diet, but no data is yet available regarding their associated microbiota, despite that the significance of bacterial communities to fish health and adaptation is increasingly acknowledged. In order to document microbiota in key fish groups from the Southern Ocean, the bacterial communities associated with the gut, fin, gills and light organs of members of six species within the three myctophid genera Electrona, Protomyctophum and Gymnoscopelus were characterized using a 16S rRNA-based metabarcoding approach. Gut communities display limited diversity of mostly fish-specific lineages likely involved in food processing. Fin and skin communities display diversity levels and compositions resembling more those found in surrounding seawater. Community compositions are similar between genera Electrona and Protomyctophum, that differ from those found in Gymnoscopelus and in water. Low abundances of potentially light-emitting bacteria in light organs support the hypothesis of host production of light. This first description of myctophid-associated microbiota, and among the first on fish from the Southern Ocean, emphasizes the need to extend microbiome research beyond economically-important species, and start addressing ecologically-relevant species.
Citation: Gallet A, Koubbi P, Léger N, Scheifler M, Ruiz-Rodriguez M, Suzuki MT, et al. (2019) Low-diversity bacterial microbiota in Southern Ocean representatives of lanternfish genera Electrona, Protomyctophum and Gymnoscopelus (family Myctophidae). PLoS ONE 14(12): e0226159. https://doi.org/10.1371/journal.pone.0226159
Editor: Varenyam Achal, Guangdong Technion Israel Institute of Technology, CHINA
Received: July 21, 2019; Accepted: November 20, 2019; Published: December 11, 2019
Copyright: © 2019 Gallet et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Data Availability: Raw reads were deposited into the GENBANK Sequence Read Archive (SRA) database under accession number SAMN12077264 to SAMN12077346, belonging to the BioProject PRJNA531247.
Funding: The cruise was operated under the auspices of IPEV and MESOPP (H2020) awarded to PK. Lab work and post-doctoral fellowship (MRR) were funded through a Sorbonne Universités EMERGENCE program MICROFISH (SU-16-R-EMR-22-MICROFISH) awarded to SD and YD. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Microbiota plays multiple fundamental roles in animal biology, including nutrition, immunity, protection and behavior . The study of microbiota in teleost fish is an emerging research topic, initially owing to its relevance to aquaculture and fisheries research [2,3]. Teleosts have also emerged as good models to investigate vertebrate host-symbiont relationships because they are easy to rear, and display relatively limited bacterial diversity compared to other vertebrates, in particular endotherms. Representing half of the vertebrate species, teleosts as a group experience a broad diversity of environmental conditions and life histories, and are thus good candidates to study how microbiota may contribute to host adaptation and resilience .
Myctophids are among the most dominant mesopelagic teleost fishes worldwide and are the most dominant in the Southern Ocean [5–7]. An estimated 24 species of Myctophidae strictly occur in the Southern Ocean while 44 more species are occasionally recorded south of the Subtropical Front . They feed on crustaceans, mostly copepods, amphipods and euphausids [8,9], and are important prey items for larger fauna, in particular mammals (seals) and birds (penguins). The Southern Ocean is one of the most extreme marine environments, most notably due to low temperature and isolation from other water masses, resulting in a low diversity of teleosts [6,10]. Teleost adaptation to cold waters has been studied in particular for the endemic Southern Ocean Notothenioidei , but very little is known regarding fish-associated microbiota in this environment despite their significance to fish physiology and ecology is well-established [2,3]. To our knowledge, two studies have investigated intestine-associated bacteria using culture-independent methods in four nothothenioid species, in Chionodraco hamatus and in Gymnodraco acuticeps [11,12]. No study to date has investigated the microbiota associated with the Myctophidae family, and generally very little is known regarding their nutrition. Their diet implies an ability to degrade large amounts of arthropod cuticle, and high levels of chitinolytic activities were indeed measured in the gut from several species, but these originated from the Monterey Bay, and not the Southern Ocean . Interestingly, Myctophidae are referred to as ‘lanternfish’ owing to their production of light. Light emission in metazoans can be of either animal or bacterial origin, the latter through symbiotic interactions . While early works found positive response to bacterial luminescence gene probes, supporting a bacterial origin for this emission, following work invalidated these results and suggested the absence of bacteria-related luciferase genes and activity in Myctophidae . This supports a metazoan origin of light emission, yet the mechanism has not been clearly elucidated and a molecular investigation of bacteria potentially associated to light organs is still lacking.
Given the ecological importance of Myctophidae in the Southern Ocean and general lack of data, this family is a good target group to investigate the composition, organ-specificity and variability of microbiota associated with Southern Ocean fish. In this study, the microbiota associated with species belonging to three genera, namely Electrona, Protomyctophum and Gymnoscopelus, was characterized. The genus Electrona is the most numerically abundant , and E. antarctica is the most abundant mesopelagic species endemic to the Southern Ocean [6,17]. Fish were sampled in the region between Crozet and Kerguelen islands where the three genera co-occur. The area is under the influence of three major fronts, the subtropical front, the subantarctic front and the Antarctic polar fronts which all influence myctophid assemblages from the subtropical zone to the subantarctic one and the Antarctic waters [6,18]. A 16S rRNA-based metabarcoding approach was used to identify and compare the bacterial taxa occurring on the gills, the fins, in the luminous organ and in the intestine of fishes. Bacterial communities present in the surrounding water were analyzed and compared with fish microbiota. Altogether, this study provides the first assessment of microbiota composition in Myctophidae species, and one of the first investigation of Antarctic fish microbiota.
Material and methods
Samples were acquired within the program VT155 REPCCOAI conducted during cruise MD206/ObsAustral aboard the RV “Marion Dufresne”, from 8 stations in the area between Crozet islands and Kerguelen (Table 1 and Fig 1) . Individuals of Electrona antarctica (10 specimens), Protomyctophum bolini and P. tenisoni (7 and 4 specimens, respectively), Gymnoscopelus bolini and G. braueri (3 specimens each) were sampled using an IKMT (Isaacs Kidd Midwater Trawl) trawled from the surface to different depths at a speed between 2 to 3 knots (Table 1). The net was 17 m long with a mesh size decreasing from its mouth (4cm) to the cod end where the mesh was 0.5 cm.
Crozet islands are located on the west, not visible. Map obtained using Google Earth.
Upon recovery, fish were immediately measured, photographed and dissected using sterile scalpels and tweezers. Caudal fins were sampled, light organs as well as two branchial arcs were dissected. The full intestine (without stomach) was sampled, its content was removed with sterile water pouring to focus on gut-associated communities and avoid bias due to the transient community occurring in the gut contents of different specimens. Samples were frozen immediately in liquid nitrogen then stored at -80°C. Water was sampled from 3 stations, including two where fish were also sampled (IK2017-14 and -18), using Niskin bottles at three depths (125, 600 and 1000 m). Upon recovery, 1L water was filtered on a 0.22 μm nitrocellulose filter and filters were frozen.
No endangered species were harvested for this study. All necessary authorizations and approval of the study protocol were obtained from the “Réserve naturelle des Terres Australes Françaises” (TAAF) prior to the cruise. Réserve nationale naturelle des Terres Australes Françaises” and TAAF administration agreed on the project. The natural reserve is a government board having a committee for environmental protection and a scientific council. PK is a member of the TAAF Scientific Committee.
DNA extraction and 16S rRNA-based metabarcoding of bacterial communities
DNA was extracted using the QIAGEN Blood and Tissue Kit according to the manufacturer’s instructions (Qiagen, CA), and visualized on an agarose gel. A fragment of the 16S rRNA-encoding gene corresponding to the V4-V5 variable region of Escherichia coli was amplified using primers 341F (5’- CCTACGGGNGGCWGCAG-3’) and 805R (5’- GACTACHVGGGTATCTAATCC-3’) [20,21] with Illumina adapters and 8-bp barcodes. The PCR mix contained 1X KAPA2G Fast Ready Mix (Sigma-Aldrich, France), 0.2 μl of each primer (concentration of 0.2 μM), 3.6 μl of ultrapure water and 1 μl of DNA in a final volume of 10 μl. After 3 min of initial denaturation at 95˚C, the PCR was run for 22 cycles (95˚C for 45s, 50˚C for 45s, and 68˚C for 90s), with a final extension step (68˚C for 5 min). Three parallel PCR reactions were run on each sample and then pooled together. PCR products were purified (USB ExoSAP-IT PCR Product Cleanup Kit from Thermofisher, France) and the DNA from different reactions was normalized with the SequalPrep Normalization Plate Kit (96 well, Thermofisher, France), and amplicons were pooled and concentrated by using the Wizard SV Gel and PCR Clean up Kit (Promega, France). Amplicons were sequenced on an Illumina® HiSeq 2500 platform (2×300 paired-end) by FASTERIS SA, Switzerland, in parallel with other projects. Raw reads were deposited into the GENBANK Sequence Read Archive (SRA) database under accession number SAMN12077264 to SAMN12077346, belonging to the BioProject PRJNA531247.
Analysis were performed using the QIIME2 software . Raw reads were demultiplexed, quality checked and trimmed to remove primer regions, paired ends were assembled, chimeric sequences were discarded, and reads were denoised using DADA2 resulting in a list of Amplicon Sequence Variants (ASVs) . Taxonomic affiliations were obtained by the sklearn-based classifier using the SILVA_132_QIIME_release distributed by the Silva project . Sequences matching “Archaea”, “Eukaryota”, “Unassigned”, “Chloroplast” and “Mitochondria”, representing 2.8% of raw reads, were discarded.
Rarefaction curves, alpha and beta diversity indexes were generated using a sampling depth of 1,100 corresponding to the lowest number of quality-filtered reads obtained in a sample. A guide phylogenetic tree was produced to compute UniFrac distances and a principal-coordinates analysis (PCoA) plot based on Weighted UniFrac (WU) dissimilarities was generated . Community richness estimated by Faith’s Phylogenetic Diversity (PD) were compared using Kruskal Wallis tests, and compositions were compared using PERMANOVA. Venn diagrams were drawn using the web-based software available at http://bioinformatics.psb.ugent.be/webtools/Venn/.
A total of 1,258,379 assembled paired-end bacterial reads were obtained from 61 fish samples (intestine, light organ, fin and gill) and 11 filtered seawater samples (Table 1). These represented 1,683 distinct ASVs. Individual samples yielded between 1,609 and 61,543 reads (mean 18,505). Numbers of reads were sometimes low, leading us to choose a minimal 1,100 reads level for rarefaction-based analyses. At this level, rarefaction curves reached saturation for animal samples at this level, while water samples did not (S1 Fig). It is thus likely that the majority of animal-associated bacterial diversity was successfully captured. At this level, between 2 and 205 (mean 48) ASVs were observed in individual samples (Table 1).
Diversity and composition of bacterial communities
Water samples displayed highest ASVs diversity with average 137.2±56.3 ASVs, followed by fin and gill samples (mean 40.1±23.6 (24 samples) and 37.5±32.0 (19 samples), respectively; see Table 2 for mean values according to host genus). Light organs displayed on average 25.4±7.9 ASVs (5 samples). Intestine samples displayed markedly lower diversity, with average 10.5±9.9 ASVs (13 samples). Faith’s PD, which accounts for the phylogenetic distance among observed ASVs, was significantly higher in water compared to all fish samples (p<0.001, S1 Table). Gymnoscopelus samples displayed a PD comparable to that of water (p = 0.78), while both Electrona and Protomyctophum samples displayed markedly lower PDs (both p-values versus water <0.001), comparable between them (Electrona versus Protomyctophum samples, p = 0.62).
Among fish organs, light organs were excluded from alpha diversity comparisons because only 5 samples were analyzed. Fin and gill samples were found to display comparable PDs (p = 0.85), both well above those in intestine samples (both p-values versus intestine <0.001). Sampling date did not affect Faith PD (p = 0.72).
The two most abundant bacterial groups in all fish samples were Gammaproteobacteria (notably Alteromonadales, Pseudomonadales, Thiomicrospirales and, to a lesser extent, Vibrionales) and Mollicutes (Mycoplasmatales, Fig 2). In the light organ, dominant ASVs belonged to the Mycoplasmatales (41.3±37.4%, notably genus Mycoplasma), Alteromonadales (22.2±29.5%, genus Pseudoalteromonas), and Pseudomonadales (22.3±32.8%, genus Acinetobacter), and abundances were variable across samples. In intestine samples, Mollicutes were consistently dominant in all samples of Electrona antarctica (97.9±4.1% of reads). Mollicutes were also abundant in intestine samples of Protomyctophum (mean 29.2±43.6%) but Thiomicrospirales (27.6±40.9%), including two ASVs belonging to the clade SUP-05 of sulfur-oxidizing bacteria, and Vibrionales (13.7±23.1%) represented by two ASVs within genus Vibrio present in one sample each, were also abundant in some samples. Despite that several ASVs belonging to the Mollicutes and Gammaproteobacteria were present, a single ASV sometimes represented up to 99% of reads, emphasizing the overall low bacterial diversity in intestine samples (S2 Table). Fin and gill samples displayed dominance of Gammaproteobacteria (68.6±6.2% and 81.6±5.9%, respectively) and Mollicutes (19.1±33.2% and 13.0±27.7%, respectively), with a greater diversity of ASVs compared to other animal sample types. Water samples were dominated by Proteobacteria of the Gamma, Alpha and Delta groups, and Mollicutes represented less than 0.1% of reads in any of the water sample.
Among abundant ASVs, i.e. the 217 representing at least 1% of reads in at least one sample, 53 were shared between at least two genera, or a genus and water. Ten out of the 67 abundant ASVs in water were shared with fish, 7 of which were shared with all three fish genera, and 6 ASVs (all belonging to the Gammaproteobacteria) were shared with all four organ types (Fig 3 left). The three fish genera shared 19 additional ASVs (including 15 Gammaproteobacteria) that were not abundant in water samples. Protomyctophum and Electrona shared additional 14 ASVs that were absent in Gymnoscopelus (11 Gammaproteobacteria and 3 Mollicutes), while the latter genus shared only 5 exclusive ASVs with either of the former two, suggesting a greater similarity between microbiota of Protomyctophum and Electrona. When comparing organs, 81 ASVs were shared between at least two organs or organ and water. These included the 6 gammaproteobacterial ASVs all organs shared with water, and 16 ASVs that were shared among all organs but absent in water samples (including 11 Gammaproteobacteria and 4 Mollicutes; Fig 3 right).
Venn diagrams displaying the number of shared ASVs among the myctophid genera (left) and organs (right). Only ASVs representing at least 1% of reads in at least one sample are included.
In order to compare community compositions, Weighted UniFrac (WU) distances were chosen to account for both phylogenetic proximity among ASVs as well as their relative abundances. Two samples (one fin and one gill) from G. braueri displayed extremely large distances with all other samples in the exploratory analyses and were removed based on information from further plots and comparisons identifying them as outliers. Water samples formed a tight cluster in the WU PCoA plot compared to fish samples (Fig 4). Samples from the genera Electrona and Protomyctophum occupied overlapping regions on the graph, while Gymnoscopelus samples were spread over the whole graph, suggesting higher variability in the latter (Fig 4).
Colors correspond to water (blue) and genera Electrona (yellow), Gymnoscopelus (red) and Protomyctophum (green); and shapes to gill (diamond), fin (cone), and intestine (square). Light organs as well as two outliers were not included (see text).
Statistical comparisons of fish-associated community compositions were performed at the fish genus level. Light organ samples were not included because only 5 samples were available, and n = 1 for two of the genera. PERMANOVA followed by pairwise tests (S1 Table) revealed that communities from Electrona and Protomyctophum did not display significantly different compositions (p = 0.12), while both differed from water samples (p-values<0.01). Gymnoscopelus samples differed from the two other fish genera (both p-values<0.05) and from water (p = 0.002 and p = 0.003, respectively). Unfortunately, no intestine sample was available, and sample composition was highly variable, so the results for Gymnoscopelus are to be treated with caution. Community compositions in the different organs were also compared. Gill and fin displayed highly similar compositions (p = 0.77), significantly different from that of water samples (both p-values = 0.001). Intestine-associated bacterial community compositions differed significantly from those of gill, fin and water samples (p-values = 0.001). No significant difference was found in community compositions among the different sampling dates (p = 0.13).
Low bacterial diversity in the intestine of myctophid fish
Fish body parts displayed markedly lower ASV diversity compared to water samples. Notably, the lowest diversity was observed in the intestine samples, with intermediate values in the fins and gills that are in contact with the environment (see below). Phylogenetic diversity followed the same trend. As the latter accounts for evolutionary distances among ASVs, it can be assumed that higher values suggest a more functionally-diverse community . It is thus likely that lower values in intestine samples reflect a narrower taxonomical and functional diversity compared to fins, gills and light organs, and to water. Lower diversity in the gut versus environment-exposed tissues is commonly reported in vertebrate microbiome studies, possibly because of the occurrence of digestive enzymes, and low pH which make for a more stressful habitat, although fish guts displays higher oxygen levels than endotherm guts .
Whether the alpha diversity levels observed here and in Southern Ocean fishes in general are overall lower than in fishes from less extreme (e.g. warmer) environments is hard to say at this stage because of the lack of data in this region. A study based on clone libraries (~500 clones analyzed) for example revealed only 17 and 6 OTUs in the gut of notothenioid fishes Notothenia coriiceps and Chaenocephalus aceratus, respectively, with dominance of gammaproteobacterial genera Photobacterium, Vibrio and Aliivibrio and estimated coverage above 96% . Sedlacek isolated 38 strains of Enterobacter and 6 of Aeromonas from 4 Notothenioidei fish species but did not provide any estimate of their relative abundance . A recent study on 4 species (Trematomus bernacchii and Pagothenia borchgrevinki (family Nototheniidae), Chionodraco hamatus, (family Channichthyidae) and Gymnodraco acuticeps (family Bathydraconidae) analyzed the gut content microbiota and showed a predominance of Proteobacteria, Actinobacteria and Firmicutes, yielding several hundred OTUs per sample (yet without exact numbers provided ).
Most previous studies, including those discussed above, have used Operational Taxonomic Units (OTUs) for sequence reads clustering instead of ASVs. ASVs have emerged recently as a more appropriate mean of evaluating microbial diversity , but on the other hand diversity metrics inferred from the two approaches are hard to directly compare. A recent work in our group on laboratory-reared medaka Oryzias latipes using a similar approach revealed an average of 95 ASVs in gut samples, suggesting that myctophid fish from the present study display a much lower bacterial diversity in their intestine . In a recent analysis of rainbow trouts (Oncorhynchus mykiss) in an aquaculture setting, between 15 and 29 ASVs were identified in the gut, slightly above values reported here, with a dominance of Mycoplasmatales as found here . The paucity of literature regarding Southern Ocean fish microbiota does not allow direct comparison, and it is possible that a fraction of the diversity was missed using our approach due to relatively low total numbers of reads in certain samples, yet overall it seems that myctophids from this study display a low diversity of bacteria in their intestine compared to other fish in which comparable analyses were conducted.
The gill and fins display specific bacterial communities at the interface between fish and seawater
The intestine-associated bacterial community differed from that of the seawater, but interestingly, also from that of gill and fins, as previously reported in the rainbow trout . The latter two, dominated by Gammaproteobacteria and Mollicutes, were also significantly different from seawater communities, emphasizing the peculiarities of surface epithelia and associated mucus, sit at the interface between seawater and hosts [29,31]. Proteobacteria are reported as dominant members of the gill and skin-associated communities of numerous teleosts, including for example the seabass Dicentrarchus labrax and seabream Sparus aurata [2,32]. In the present study, we analyzed fins instead of fish skin because the latter was often damaged during fishing operations. Although skin and fins likely represent similar habitats, some work has shown that differences could exist between associated communities that may reflect stochastic effects. Nevertheless, in one study, Proteobacteria were found dominant in both fin as well as skin samples of D. labrax and S. aurata . The mucus covering gill and fins surfaces has a protective role, and acts as a filter and first line of defense against parasites and pathogens. However, the abundance of organic substrates available to heterotrophic microorganisms may on the other hand attract various microorganisms not necessarily abundant in surrounding water, and is, to a certain extent permissive to bacterial colonization, allowing a diversity of bacteria to establish . Brown et al. reported 50 to 57 ASVs in the gills of Oncorhynchus mykiss, with dominance of Proteobacteria, in the range of values reported here , while reports on the seabass and seabream recently indicated higher diversity (457 to 539 ASVs, with 2 to 24 belonging to the core microbiota) . Bacterial diversity thus seems to vary greatly among species, and it is hard to conclude whether the diversity level observed in Myctophidae gills and fins should be considered low.
Significance of microbiota composition to myctophid biology and ecology
Dominant members of fish-associated communities included various Mycoplasmataceae (Mollicutes), while none was abundant in water samples. Mycoplasmataceae are commonly reported as abundant in fish microbiota studies, notably in several omnivorous (e.g. Gillichthys mirabilis and Lagodon rhomboides) and carnivorous species (e.g. Salmo salar, Sciaenops ocellatus) . They for example dominate in all salmonid species investigated to date, including wild and farmed [29,30,34]. In these, an antagonism apparently exists between Mycoplasma and pathogenic Vibrio, suggesting that the former prevents the establishment of the pathogen . Mycoplasma are also dominant in the gut of farmed rainbow trouts in which they are likely fermenting various substrates and contributing the host lactic and acetic acid . Interestingly, Mycoplasma were most abundant in trout fed with insect-enriched diets, and chitin was suggested as a prebiotic. Similarly, the arthropod-based, chitin-rich diet of Myctophidae may favor dominance of Mycoplasma in specimens from our study. Overall, for these reasons, it can be hypothesized that Mycoplasma could be beneficial partners in a long-established symbiosis with fish guts.
Interestingly, members of the Vibrionales and the genus Vibrio, while usually important members of fish microbiota with diverse functions ranging from pathogenic to probiotic , were not abundant in fish samples, except in a few samples of Protomyctophum, and were almost completely absent in Electrona samples. This is congruent with the aforementioned antagonism hypothesis, and suggests a pathogenic status for identified Vibrionales ASVs, with high abundances corresponding to infected individuals. The presence of members of the SUP-05 cluster in the intestine, gill and fins of several specimens of Protomyctophum, with sometimes high abundances, is also intriguing. This bacterial clade indeed includes mostly aerobic, sulfur-oxidizing autotrophic bacteria, some members being symbiotic with deep-sea metazoans from seeps and vents .
Addressing the role of microbiota for Myctophidae is thus not straightforward at this stage. Regarding nutrition, Myctophidae consume mainly copepods, euphausiids, pteropods and hyperiids, and some non-Antarctic species within this family display high levels of chitinolytic enzymes . Pakhomov pointed no substantial differences in the regime, based on prey availability rather than selection, among 36 species including three from the present study . Recently however, some level of trophic niche differenciation was suggested among members of the genera Electrona, Gymnoscopelus and Protomyctophum sampled from around the Kerguelen Islands, including all 5 species from the present study . Gymnoscopelus bolini and G. braueri for example displayed higher δ15N signatures, indicative of higher trophic level compared to Electrona antarctica and Protomyctophum species. Interestingly, Gymnoscopelus-associated bacterial communities tend to differ from those in Electrona and Protomyctophum here, however at this stage the link between microbiota composition and trophic level cannot be tested. Another trait that may involve bacteria is bioluminescence . Myctophid fish are indeed known to emit bioluminescence in their ventral and lateral light organs. While early works suggested a bacterial origin for this emission, following work rather pointed towards the metazoan origin of the process [38,39]. We specifically investigated for the presence of ASVs corresponding to two reportedly light-producing bacterial genera, Aliivibrio and Photobacterium (8 and 1 ASVs, respectively) in light organ samples of Gymnoscopelus and Protomyctophum. None was above 2.5% of reads, supporting previous reports that indicate that bioluminescence in this teleost family is not due to a bacterial symbiosis [15,39].
In conclusion, this study shows that Gammaproteobacteria and Mollicutes are the dominant bacterial taxa present in the intestine, fin, gill and light organs of three genera of plankton-feeding Myctophidae. Electrona, the most abundant genus in the Southern Ocean, and Protomyctophum display overall similar microbiota compositions while that of Gymnoscopelus is apparently different but warrants further study because of the low number of samples included in this study. The intestine-associated microbiota displays low diversity and is different from that of gills and fins, with a dominance of Mollicutes in particular in Electrona. The overall rarity of Vibrionales is to be noted, as is the occurrence of members of the clade SUP-05 in Protomyctophum. Potential light-emitting bacteria were almost absent from light organs. These findings provide the first assessment of microbiota composition in the most abundant fish family from the Southern Ocean. However, in this study, sampling was performed over a short period of time, and the existence of seasonal variation in microbiota composition should be further monitored throughout the year. To test whether low diversity is a specificity of the family Myctophidae or is due to their extreme Southern Ocean habitat, it will be necessary to perform similar analyses on species that are not endemic to the Southern Ocean. Finally, the next step will be to investigate the roles of Myctophidae microbiota using functional approaches, in order to evaluate the role of microbiota in host biology and nutrition.
S1 Fig. Rarefaction curves by sample type, indicating that samples of animal origin (gill, fin, intestine and luminous organ) reach saturation at the selected 1,100 sequencing depth. Water samples do not reach saturation and associated diversity is thus likely underestimated.
S1 Table. Results from Kruskal-Wallis tests done on Faith Phylogenetic Diversity (sheet 1) and PERMANOVA analyses (sheet 2) conducted to test the effect of genus, tissue and date, and associated pairwise tests.
P-values < 0.05 are in bold.
We thank crew and scientists involved in the cruise, in particular J-Y Toullec and B. Leroy. Field and lab work. We are grateful to the BIO2MAR platform (http://bio2mar.obs-banyuls.fr) for technical help in the preparation of samples for sequencing.
- 1. McFall-Ngai M, Hadfield MG, Bosch TCG, Carey HV, Domazet-Loso T, Douglas AE, et al. Animals in a bacterial world, a new imperative for the life sciences. Proc Natl Acad Sci U S A. 2013;110: 3229–3236. pmid:23391737
- 2. Llewellyn MS, Boutin S, Hoseinifar SH, Derome N. Teleost microbiomes: the state of the art in their characterization, manipulation and importance in aquaculture and fisheries. Front Microbiol. 2014;5. pmid:24917852
- 3. Egerton S, Culloty S, Whooley J, Stanton C, Ross RP. The Gut Microbiota of Marine Fish. Front Microbiol. 2018;9. pmid:29780377
- 4. Lescak EA, Milligan-Myhre KC. Teleosts as Model Organisms To Understand Host-Microbe Interactions. J Bacteriol. 2017;199. pmid:28439034
- 5. Cherel Y, Fontaine C, Richard P, Labat J-P. Isotopic niches and trophic levels of myctophid fishes and their predators in the Southern Ocean. Limnol Oceanogr. 2010;55: 324–332.
- 6. Duhamel G, Hulley PA, Causse R, Koubbi P, Vacchi M, Pruvost P, et al. Biogeographic patterns of fish. Biogeographic atlas of the Southern Ocean. Cambridge, UK: De Broyer C., Koubbi P., Griffith H.J., Raymond B., Udekem d’Acoz C. et al (eds); 2014. pp. 328–362.
- 7. Saunders RA, Collins MA, Ward P, Stowasser G, Shreeve R, Tarling GA. Distribution, population structure and trophodynamics of Southern Ocean Gymnoscopelus (Myctophidae) in the Scotia Sea. Polar Biol. 2015;38: 287–308.
- 8. Pakhomov EA, Perissinotto R, McQuaid CD. Prey composition and daily rations of myctophid fishes in the Southern Ocean. Mar Ecol Prog Ser. 1996;134: 1–14.
- 9. Saunders RA, Collins MA, Ward P, Stowasser G, Hill SL, Shreeve R, et al. Predatory impact of the myctophid fish community on zooplankton in the Scotia Sea (Southern Ocean). Mar Ecol Prog Ser. 2015;541: 45–64.
- 10. Eastman JT. The nature of the diversity of Antarctic fishes. Polar Biol. 2005;28: 93–107.
- 11. Ward NL, Steven B, Penn K, Methe BA, Detrich WH. Characterization of the intestinal microbiota of two Antarctic notothenioid fish species. Extremophiles. 2009;13: 679–685. pmid:19472032
- 12. Song W, Li L, Huang H, Jiang K, Zhang F, Chen X, et al. The Gut Microbial Community of Antarctic Fish Detected by 16S rRNA Gene Sequence Analysis. In: BioMed Research International [Internet]. 2016 [cited 21 May 2019]. pmid:27957494
- 13. Gutowska MA, Drazen JC, Robison BH. Digestive chitinolytic activity in marine fishes of Monterey Bay, California. Comp Biochem Physiol -Mol Integr Physiol. 2004;139: 351–358. pmid:15556391
- 14. Widder EA. Bioluminescence in the Ocean: Origins of Biological, Chemical, and Ecological Diversity. Science. 2010;328: 704–708. pmid:20448176
- 15. Deshmukh A. Control of bioluminescence in Myctophid fishes. IJMS Vol4607 July 2017. 2017; Available: http://nopr.niscair.res.in/handle/123456789/42233
- 16. Collins MA, Stowasser G, Fielding S, Shreeve R, Xavier JC, Venables HJ, et al. Latitudinal and bathymetric patterns in the distribution and abundance of mesopelagic fish in the Scotia Sea. Deep Sea Res Part II Top Stud Oceanogr. 2012;59–60: 189–198.
- 17. Hulley PA. Myctophidae. Grahamstown: J.L.B. Smith Institute of Ichthyology.; 1990.
- 18. Koubbi P, Moteki M, Duhamel G, Goarant A, Hulley P-A, O’Driscoll R, et al. Ecoregionalization of myctophid fish in the Indian sector of the Southern Ocean: Results from generalized dissimilarity models. Deep Sea Res Part II Top Stud Oceanogr. 2011;58: 170–180.
- 19. Toullec JY, Koubbi P. VT 155 / REPCCOAI Cruise, RV Marion Dufresne [Internet]. 2017. Available: https://doi.org/10.17600/17017100
- 20. Klindworth A, Pruesse E, Schweer T, Peplies J, Quast C, Horn M, et al. Evaluation of general 16S ribosomal RNA gene PCR primers for classical and next-generation sequencing-based diversity studies. Nucleic Acids Res. 2013;41: e1. pmid:22933715
- 21. Sinclair L, Osman OA, Bertilsson S, Eiler A. Microbial Community Composition and Diversity via 16S rRNA Gene Amplicons: Evaluating the Illumina Platform. PLOS ONE. 2015;10: e0116955. pmid:25647581
- 22. Hall M, Beiko RG. 16S rRNA Gene Analysis with QIIME2. Methods Mol Biol Clifton NJ. 2018;1849: 113–129. pmid:30298251
- 23. Callahan BJ, McMurdie PJ, Holmes SP. Exact sequence variants should replace operational taxonomic units in marker-gene data analysis. ISME J. 2017;11: 2639. pmid:28731476
- 24. Pruesse E, Quast C, Knittel K, Fuchs BM, Ludwig W, Peplies J, et al. SILVA: a comprehensive online resource for quality checked and aligned ribosomal RNA sequence data compatible with ARB. Nucleic Acids Res. 2007;35: 7188–7196. pmid:17947321
- 25. Lozupone C, Knight R. UniFrac: a new phylogenetic method for comparing microbial communities. Appl Environ Microbiol. 2005;71: 8228–8235. pmid:16332807
- 26. Faith DP. Conservation evaluation and phylogenetic diversity. Biol Conserv. 1992;61: 1–10.
- 27. Sedlacek I, Stankova E, Svec P. Composition of cultivable enteric bacteria from the intestine of Antarctic fish (family Nototheniidae). Czech J Anim Sci. 2016;61: 127–132.
- 28. Duperron S, Halary S, Habiballah M, Gallet A, Huet H, Duval C, et al. Response of Fish Gut Microbiota to Toxin-Containing Cyanobacterial Extracts: A Microcosm Study on the Medaka (Oryzias latipes). Environ Sci Technol Lett. 2019;6: 341–347.
- 29. Brown RM, Wiens GD, Salinas I. Analysis of the gut and gill microbiome of resistant and susceptible lines of rainbow trout (Oncorhynchus mykiss). Fish Shellfish Immunol. 2019;86: 497–506. pmid:30513381
- 30. Lowrey L, Woodhams DC, Tacchi L, Salinas I. Topographical Mapping of the Rainbow Trout (Oncorhynchus mykiss) Microbiome Reveals a Diverse Bacterial Community with Antifungal Properties in the Skin. Appl Environ Microbiol. 2015;81: 6915–6925. pmid:26209676
- 31. Kelly C, Salinas I. Under Pressure: Interactions between Commensal Microbiota and the Teleost Immune System. Front Immunol. 2017;8: 559. pmid:28555138
- 32. Rosado D, Pérez-Losada M, Severino R, Cable J, Xavier R. Characterization of the skin and gill microbiomes of the farmed seabass (Dicentrarchus labrax) and seabream (Sparus aurata). Aquaculture. 2019;500:57–64.
- 33. Chiarello M, Villéger S, Bouvier C, Bettarel Y, Bouvier T. High diversity of skin-associated bacterial communities of marine fishes is promoted by their high variability among body parts, individuals and species. FEMS Microbiol Ecol. 2015;91: fiv061. pmid:26048284
- 34. Holben WE, Williams P, Gilbert MA, Saarinen M, Särkilahti LK, Apajalahti JHA. Phylogenetic analysis of intestinal microflora indicates a novel Mycoplasma phylotype in farmed and wild salmon. Microb Ecol. 2002;44: 175–185. pmid:12082453
- 35. Ciric M, Waite D, Draper J, Jones JB. Characterisation of gut microbiota of farmed Chinook salmon using metabarcoding. bioRxiv. 2018; 288761.
- 36. Rimoldi S, Gini E, Iannini F, Gasco L, Terova G. The effect of dietary insect meal from Hermetia illucens prepupae on autochtonous gut microbiota of Rainbow trout (Oncorhynchus mykiss). Animals. 2019;9:143. pmid:30987067
- 37. Dubilier N, Bergin C, Lott C. Symbiotic diversity in marine animals: the art of harnessing chemosynthesis. Nat Rev Microbiol. 2008;6: 725–740. pmid:18794911
- 38. Foran D. Evidence of luminous bacterial symbionts in the light organs of myctophid and stomiiform fishes. J Exp Zool. 1991;259: 1–8. pmid:2072087
- 39. Haygood M, Edwards D, Mowlds G, Rosenblatt R. Bioluminescence of Myctophid and Stomiiform Fishes Is Not Due to Bacterial Luciferase. J Exp Zool. 1994;270: 225–231.