Abstract
Bivalves have ecological and economic importance but information regarding their associated microbiomes is lacking. As suspension feeders, bivalves capture and ingest a myriad of particles, and their digestive organs have a high throughput of particle-associated microbiota. To better understand the complement of transient and resident microbial communities, standard methods need to be developed. For example, fecal sampling could represent a convenient proxy for the gut microbiome and is simple, nondestructive, and allows for sampling of individuals through time. The goal of this study was to evaluate fecal sampling as a reliable proxy for gut microbiome assessment in the blue mussel (Mytilus edulis). Mussels were collected from the natural environment and placed into individual sterilized microcosms for 6 h to allow for fecal egestion. Feces and gut homogenates from the same individuals were sampled and subjected to 16S rRNA gene amplicon sequencing. Fecal communities of different mussels resembled each other but did not resemble gut communities. Fecal communities were significantly more diverse, in terms of amplicon sequence variant (ASV) richness and evenness, than gut communities. Results suggested a mostly transient nature for fecal microbiota. Nonetheless, mussels retained a distinct resident microbial community in their gut after fecal egestion that was dominated by ASVs belonging to Mycoplasma. The use of fecal sampling as a nondestructive substitute for direct sampling of the gut is strongly discouraged. Experiments that aim to study solely resident bivalve gut microbiota should employ an egestion period prior to gut sampling to allow time for voidance of transient microbes.
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Availability of Data and Material
The data from this work are available upon email request from Tyler W. Griffin. Sequence data were uploaded to the NCBI Short Read Archive (SRA) under submission ID SUB7223904 (BioProject ID: PRJNA622268).
References
Dame R (1993) Bivalve filter feeders and estuarine and coastal ecosystem processes: conclusions. Bivalve Filter Feeders. Springer, pp 565–569
Prins TC, Smaal AC, Dame RF (1998) A review of the feedbacks between bivalve grazing and ecosystem processes. Aquat Ecol 31:349–359. https://doi.org/10.1023/A:1009924624259
Newell RIE (2004) Ecosystem influences of natural and cultivated populations of suspension-feeding bivalve molluscs: a review. J Shellfish Res 23:51–61
Cranford PJ, Ward JE, Shumway SE (2011) Bivalve filter feeding: variability and limits of the aquaculture biofilter. In: Shumway SE (ed) Shellfish aquaculture and the environment 1st edn. Wiley, pp 81–124
Hammer TJ, Sanders JG, Fierer N (2019) Not all animals need a microbiome. FEMS Microbiol Lett 366:366. https://doi.org/10.1093/femsle/fnz117
Yatsunenko T, Rey FE, Manary MJ, Trehan I, Dominguez-Bello MG, Contreras M, Magris M, Hidalgo G, Baldassano RN, Anokhin AP, Heath AC, Warner B, Reeder J, Kuczynski J, Caporaso JG, Lozupone CA, Lauber C, Clemente JC, Knights D, Knight R, Gordon JI (2012) Human gut microbiome viewed across age and geography. Nature 486:222–227. https://doi.org/10.1038/nature11053
Aagaard K, Petrosino J, Keitel W, Watson M, Katancik J, Garcia N, Patel S, Cutting M, Madden T, Hamilton H, Harris E, Gevers D, Simone G, McInnes P, Versalovic J (2013) The human microbiome project strategy for comprehensive sampling of the human microbiome and why it matters. FASEB J 27:1012–1022. https://doi.org/10.1096/fj.12-220806
Smits LP, Bouter KEC, de Vos WM, Borody TJ, Nieuwdorp M (2013) Therapeutic potential of fecal microbiota transplantation. Gastroenterology 145:946–953. https://doi.org/10.1053/j.gastro.2013.08.058
Durbán A, Abellán JJ, Jiménez-Hernández N, Ponce M, Ponce J, Sala T, D’Auria G, Latorre A, Moya A (2011) Assessing gut microbial diversity from feces and rectal mucosa. Microb Ecol 61:123–133. https://doi.org/10.1007/s00248-010-9738-y
Ingala MR, Simmons NB, Wultsch C, Krampis K, Speer KA, Perkins SL (2018) Comparing microbiome sampling methods in a wild mammal: fecal and intestinal samples record different signals of host ecology, Evolution. Front Microbiol 9. https://doi.org/10.3389/fmicb.2018.00803
Zhou J, Nelson TM, Rodriguez Lopez C, Sarma RR, Zhou SJ, Rollins LA (2020) A comparison of non-lethal sampling methods for amphibian gut microbiome analyses. Mol Ecol Resour n/a. https://doi.org/10.1111/1755-0998.13139
Owen G (1966) Digestion. In: Wilbur KM, Yonge CM (eds) Physiology of mollusca. Academic Press, New York, pp 53–88
Simons AL, Churches N, Nuzhdin S (2018) High turnover of faecal microbiome from algal feedstock experimental manipulations in the Pacific oyster (Crassostrea gigas). Microb Biotechnol 11:848–858. https://doi.org/10.1111/1751-7915.13277
Rubiolo JA, Lozano-Leon A, Rodriguez-Souto R, Fol Rodriguez N, Vieytes MR, Botana LM (2018) The impact of depuration on mussel hepatopancreas bacteriome composition and predicted metagenome. Antonie Van Leeuwenhoek 111:1117–1129. https://doi.org/10.1007/s10482-018-1015-y
Li Y-F, Yang N, Liang X, Yoshida A, Osatomi K, Power D, Batista FM, Yang J-L (2018) Elevated seawater temperatures decrease microbial diversity in the gut of Mytilus coruscus. Front Physiol 9:839. https://doi.org/10.3389/fphys.2018.00839
Vezzulli L, Stagnaro L, Grande C, Tassistro G, Canesi L, Pruzzo C (2018) Comparative 16SrDNA gene-based microbiota profiles of the Pacific oyster (Crassostrea gigas) and the Mediterranean mussel (Mytilus galloprovincialis) from a shellfish farm (Ligurian Sea, Italy). Microb Ecol 75:495–504. https://doi.org/10.1007/s00248-017-1051-6
Pierce ML, Ward JE (2019) Gut microbiomes of the eastern oyster (Crassostrea virginica) and the blue mussel (Mytilus edulis): temporal variation and the influence of marine aggregate-associated microbial communities. mSphere 4:e00730–e00719. https://doi.org/10.1128/mSphere.00730-19
Greenberg AE, Hunt DA (1985) Laboratory procedures for the examination of seawater and shellfish. American Public Health Association, Washington DC
Apprill A, McNally S, Parsons R, Weber L (2015) Minor revision to V4 region SSU rRNA 806R gene primer greatly increases detection of SAR11 bacterioplankton. Aquat Microb Ecol 75:129–137
Callahan BJ, McMurdie PJ, Rosen MJ, Han AW, Johnson AJA, Holmes SP (2016) DADA2: high-resolution sample inference from Illumina amplicon data. Nat Methods 13:581–583. https://doi.org/10.1038/nmeth.3869https://www.nature.com/articles/nmeth.3869#supplementary-information
Quast C, Pruesse E, Yilmaz P, Gerken J, Schweer T, Yarza P, Peplies J, Glöckner FO (2012) The SILVA ribosomal RNA gene database project: improved data processing and web-based tools. Nucleic Acids Res 41:D590–D596. https://doi.org/10.1093/nar/gks1219
Callahan B (2018) Silva taxonomic training data formatted for DADA2 (Silva version 132). https://doi.org/10.5281/zenodo.1172783
Schliep KP (2010) Phangorn: phylogenetic analysis in R. Bioinformatics 27:592–593. https://doi.org/10.1093/bioinformatics/btq706
Wright ES (2015) DECIPHER: harnessing local sequence context to improve protein multiple sequence alignment. BMC Bioinformatics 16:322. https://doi.org/10.1186/s12859-015-0749-z
McMurdie PJ, Holmes S (2013) Phyloseq: an R package for reproducible interactive analysis and graphics of microbiome census data. PLoS One 8:e61217. https://doi.org/10.1371/journal.pone.0061217
Kumar S, Stecher G, Li M, Knyaz C, Tamura K (2018) MEGA X: molecular evolutionary genetics analysis across computing platforms. Mol Biol Evol 35:1547–1549. https://doi.org/10.1093/molbev/msy096
Saitou N, Nei M (1987) The neighbor-joining method: a new method for reconstructing phylogenetic trees. Mol Biol Evol 4:406–425. https://doi.org/10.1093/oxfordjournals.molbev.a040454
Tamura K, Nei M, Kumar S (2004) Prospects for inferring very large phylogenies by using the neighbor-joining method. Proc Natl Acad Sci U S A 101:11030–11035. https://doi.org/10.1073/pnas.0404206101
Felsenstein J (1985) Confidence limits on phylogenies: an approach using the bootstrap. Evolution 39:783–791. https://doi.org/10.1111/j.1558-5646.1985.tb00420.x
Love MI, Huber W, Anders S (2014) Moderated estimation of fold change and dispersion for RNA-seq data with DESeq2. Genome Biol 15. https://doi.org/10.1186/s13059-014-0550-8
McMurdie PJ, Holmes S (2014) Waste not, want not: why rarefying microbiome data is inadmissible. PLoS Comput Biol 10:e1003531. https://doi.org/10.1371/journal.pcbi.1003531
Lozupone C, Lladser ME, Knights D, Stombaugh J, Knight R (2011) UniFrac: an effective distance metric for microbial community comparison. ISME J 5:169–172. https://doi.org/10.1038/ismej.2010.133
Anderson MJ (2014) Permutational multivariate analysis of variance (PERMANOVA)Wiley StatsRef: statistics reference online. Wiley
Anderson MJ, Walsh DCI (2013) PERMANOVA, ANOSIM, and the mantel test in the face of heterogeneous dispersions: what null hypothesis are you testing? Ecol Monogr 83:557–574. https://doi.org/10.1890/12-2010.1
Dyksma S, Pjevac P, Ovanesov K, Mussmann M (2018) Evidence for H2 consumption by uncultured Desulfobacterales in coastal sediments. Environ Microbiol 20:450–461. https://doi.org/10.1111/1462-2920.13880
Weel PBV (1961) The comparative physiology of digestion in Molluscs. Am Zool 1:245–252
Menzel RW (1955) Some phases of the biology of Ostrea equestris (Say) and comparison with Crassostrea virginica (Gmelin). Inst Mar Sci 4:69–153
Owen G (1974) Feeding and digestion in the Bivalvia. In: Lowenstein O (ed) Advances in Comparative Physiology and Biochemistry. Elsevier, pp 1–35
Foster-Smith RL (1975) The effect of concentration of suspension and inert material on the assimilation of algae by three bivalves. J Mar Biol Assoc U K 55:411–418. https://doi.org/10.1017/S0025315400016027
Gagnon C, Fisher NS (1997) The bioavailability of sediment-bound Cd, Co, and Ag to the mussel Mytilus edulis. Can J Fish Aquat Sci 54:147–156. https://doi.org/10.1139/f96-256
Oliver JD, Pruzzo C, Vezzulli L, Kaper JB (2013) Vibrio species. In: Doyle M, Buchanan R (eds) Food microbiology. ASM Press, Washington, DC, pp 401–439
Park S, Yoshizawa S, Inomata K, Kogure K, Yokota A (2012) Halioglobus japonicus gen. Nov., sp. nov. and Halioglobus pacificus sp. nov., members of the class Gammaproteobacteria isolated from seawater. Int J Syst Evol Microbiol 62:1784–1789. https://doi.org/10.1099/ijs.0.031443-0
Li S-H, Song J, Lim Y, Joung Y, Kang I, Cho J-C (2020) Halioglobus maricola sp. nov., isolated from coastal seawater. Int J Syst Evol Microbiol. https://doi.org/10.1099/ijsem.0.003985
Kawasaki K, Nogi Y, Hishinuma M, Nodasaka Y, Matsuyama H, Yumoto I (2002) Psychromonas marina sp. nov., a novel halophilic, facultatively psychrophilic bacterium isolated from the coast of the Okhotsk Sea. Int J Syst Evol Microbiol 52:1455–1459. https://doi.org/10.1099/00207713-52-5-1455
Hosoya S, Jang J-H, Yasumoto-Hirose M, Matsuda S, Kasai H (2009) Psychromonas agarivorans sp. nov., a novel agarolytic bacterium. Int J Syst Evol Microbiol 59:1262–1266. https://doi.org/10.1099/ijs.0.003244-0
Yoon J, Matsuo Y, Katsuta A, Jang J-H, Matsuda S, Adachi K, Kasai H, Yokota A (2008) Haloferula rosea gen. nov., sp. nov., Haloferula harenae sp. nov., Haloferula phyci sp. nov., Haloferula helveola sp. nov. and Haloferula sargassicola sp. nov., five marine representatives of the family Verrucomicrobiaceae within the phylum ‘Verrucomicrobia’. Int J Syst Evol Microbiol 58:2491–2500. https://doi.org/10.1099/ijs.0.2008/000711-0
Nedashkovskaya OI, Kim SB, Han SK, Rhee M-S, Lysenko AM, Rohde M, Zhukova NV, Frolova GM, Mikhailov VV, Bae KS (2004) Algibacter lectus gen. nov., sp. nov., a novel member of the family Flavobacteriaceae isolated from green algae. Int J Syst Evol Microbiol 54:1257–1261. https://doi.org/10.1099/ijs.0.02949-0
Duggins DO, Eckman JE (1997) Is kelp detritus a good food for suspension feeders? Effects of kelp species, age and secondary metabolites. Mar Biol 128:489–495. https://doi.org/10.1007/s002270050115
Urbanczyk H, Ast JC, Higgins MJ, Carson J, Dunlap PV (2007) Reclassification of Vibrio fischeri, Vibrio logei, Vibrio salmonicida and Vibrio wodanis as Aliivibrio fischeri gen. nov., comb. nov., Aliivibrio logei comb. nov., Aliivibrio salmonicida comb. nov. and Aliivibrio wodanis comb. nov. Int J Syst Evol Microbiol 57:2823–2829. https://doi.org/10.1099/ijs.0.65081-0
McFall-Ngai M (2014) Divining the essence of symbiosis: insights from the squid-vibrio model. PLoS Biol 12:e1001783. https://doi.org/10.1371/journal.pbio.1001783
Nedashkovskaya OI, Kim SB, Han SK, Rhee MS, Lysenko AM, Falsen E, Frolova GM, Mikhailov VV, Bae KS (2004) Ulvibacter litoralis gen. nov., sp. nov., a novel member of the family Flavobacteriaceae isolated from the green alga Ulva fenestrata. Int J Syst Evol Microbiol 54:119–123. https://doi.org/10.1099/ijs.0.02757-0
Imhoff JF (2014) The family Chromatiaceae. In: Rosenberg E, DeLong EF, Lory S, Stackebrandt E, Thompson F (eds) The prokaryotes: Gammaproteobacteria. Springer, Berlin Heidelberg, pp 151–178
Harris JM (1993) The presence, nature, and role of gut microflora in aquatic invertebrates: a synthesis. Microb Ecol 25:195–231
Hammer TJ, Janzen DH, Hallwachs W, Jaffe SP, Fierer N (2017) Caterpillars lack a resident gut microbiome. Proc Natl Acad Sci 114:9641–9646. https://doi.org/10.1073/pnas.1707186114
King GM, Judd C, Kuske CR, Smith C (2012) Analysis of stomach and gut microbiomes of the eastern oyster (Crassostrea virginica) from coastal Louisiana, USA. PLoS One 7:e51475. https://doi.org/10.1371/journal.pone.0051475
Milan M, Carraro L, Fariselli P, Martino ME, Cavalieri D, Vitali F, Boffo L, Patarnello T, Bargelloni L, Cardazzo B (2018) Microbiota and environmental stress: how pollution affects microbial communities in Manila clams. Aquat Toxicol 194:195–207. https://doi.org/10.1016/j.aquatox.2017.11.019
King WL, Siboni N, Williams NLR, Kahlke T, Nguyen KV, Jenkins C, Dove M, O’Connor W, Seymour JR, Labbate M (2019) Variability in the composition of Pacific oyster microbiomes across oyster families exhibiting different levels of susceptibility to OsHV-1 μvar disease. Front Microbiol 10. https://doi.org/10.3389/fmicb.2019.00473
Pierce ML, Ward JE (2018) Microbial ecology of the Bivalvia, with an emphasis on the family Ostreidae. J Shellfish Res 37:1–14. https://doi.org/10.2983/035.037.0300
Murphy AE, Kolkmeyer R, Song B, Anderson IC, Bowen J (2019) Bioreactivity and microbiome of biodeposits from filter-feeding bivalves. Microb Ecol 77:343–357. https://doi.org/10.1007/s00248-018-01312-4
Kautsky N, Evans S (1987) Role of biodeposition by Mytilus edulis in the circulation of matter and nutrients in a Baltic coastal ecosystem. Mar Ecol Prog Ser 38:201–212
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This research was funded by a National Science Foundation (NSF) Research Experience for Undergraduate (REU) site grant to Mystic Aquarium and UConn; Award # 1559180.
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All authors contributed to the study conception and design. Material preparation, data collection, and analysis were performed by Julia Baer and Tyler W. Griffin. The first draft of the manuscript was written by Tyler W. Griffin and all authors commented on previous versions of the manuscript. All authors read and approved the final manuscript.
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Griffin, T.W., Baer, J.G. & Ward, J.E. Direct Comparison of Fecal and Gut Microbiota in the Blue Mussel (Mytilus edulis) Discourages Fecal Sampling as a Proxy for Resident Gut Community. Microb Ecol 81, 180–192 (2021). https://doi.org/10.1007/s00248-020-01553-2
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DOI: https://doi.org/10.1007/s00248-020-01553-2