Association between bacterial community structures and mortality of fish larvae in intensive rearing systems
Bacterial community structures were analyzed in water used for rearing fish larvae by fluorescence in situ hybridization. In Experiment 1, red sea bream Pagrus major larvae were reared in two commercial seed production tanks. The survival rate in Tank 1 was higher than in Tank 2, even though phytoplankton, Nannochloropsis sp., was added to both tanks. In Tank 2, γ-proteobacteria became dominant (∼70% of total bacteria) on day 13, there after heavy larval mortalities occurred. In Tank 1, however, α-proteobacteria and the Cytophaga-Flavobacterium cluster were predominant from day − 1 until day 13; no significant mortality was recorded. In Experiment 2, marble goby Oxyeleotris marmoratus larvae were cultured with or without Nannochloropsis sp. At the end of the experiment, larval survival rates in aquaria with Nannochloropsis sp. were significantly (P <0.05) higher than those without. In rearing water without Nannochloropsis sp., γ-proteobacteria increased during rearing. In rearing water with Nannochloropsis sp., α-prote obacteria and the Cytophaga-Flavobacterium cluster were predominant at the beginning of the experiments and the relative abundance of γ-proteobacteria was maintained at a lower level throughout the experiments. The predominance of α-proteobacteria and the Cytophaga-Flavobacterium cluster appears to be a good indicator of successful larval production.
Key Wordsbacterial community structure fluorescence in situ hybridization (FISH) larval mortality larval rearing phytoplankton
Planas M, Cunha I. Larviculture of marine fish: problems and perspectives. Aquaculture
: 171–190.CrossRefGoogle Scholar
Munro PD, Barbour A, Birkbeck TH. Comparison of the growth and survival of larval turbot in the absence of Vibrio anguillarum, Vibrio alginolyticus
, or a marine Aeromonas
sp. Appl. Environ. Microbiol.
: 4425–4428.PubMedGoogle Scholar
Skjermo J, Salvesen I, Øie G, Vadstein O. Microbially matured water: a technique for selection of a nonopportunistic bacterial flora in water that may improve performance of marine larvae. Aquacult. Int.
: 13–28.CrossRefGoogle Scholar
Salvesen I, Skjermo J, Vadstein O. Growth of turbot (Scophthalmus maximus
L.) during first feeding in relation to the proportion of r/K
-strategists in the bacterial community of the rearing water. Aquaculture
: 337–350.CrossRefGoogle Scholar
Verner-Jeffreys DW, Shields RJ, Bricknell IR, Birkbeck TH. Effects of different water treatment methods and antibiotic addition on larval survival and gut microflora development in Atlantic halibut (Hippoglossus hippoglossus
L.) yolk-sac larvae. Aquaculture
: 129–143.CrossRefGoogle Scholar
Olafsen JA. Interactions between fish larvae and bacteria in marine aquaculture. Aquaculture
: 223–247.CrossRefGoogle Scholar
Bourne DG, Young N, Webster N, Payne M, Salmon M, Demel S, Hall M. Microbial community dynamics in a larval aquaculture system of the tropical rock lobster, Panulirus ornatus
: 31–51.CrossRefGoogle Scholar
Jorquera MA, Lody M, Leyton Y, Riquelme C. Bacteria of subclass γ-Proteobacteria associated with commercial Argopecten purpuratus
(Lamark, 1819) hatcheries in Chile. Aquaculture
: 37–51.CrossRefGoogle Scholar
Tolomei A, Burke C, Crer B, Carson J. Bacterial decontamination of on-grown Artemia
: 357–371.CrossRefGoogle Scholar
Schulze AD, Alabi AO, Tattersall-Sheldrake AR, Miller KM. Bacterial diversity in a marine hatchery: balance between pathogenic and potentially probiotic bacterial strains. Aquaculture
: 50–73.CrossRefGoogle Scholar
Itoi S, Niki A, Sugita H. Changes in microbial communities associated with the conditioning of filter material in recirculating aquaculture systems of the pufferfish Takifugu rubripes
: 287–295.CrossRefGoogle Scholar
Glöckner FO, Fuchs BM, Amann R. Bacterioplankton compositions of lakes and oceans: a first comparison based on fluorescence in situ hybridization. Appl. Environ. Microbiol.
: 3721–3726.PubMedGoogle Scholar
Manz W, Amann R, Ludwig W, Wagner M, Schleifer K. Phylogenetic oligodeoxynucleotide probes for the major subclasses of proteobacteria: problems and solutions. Syst. Appl. Microbiol.
: 593–600.Google Scholar
Manz W, Amann R, Ludwig W, Vancanneyt M, Schleifer K. Application of a suite of 16S rRNA-specific oligonucleotide probes designed to investigate bacteria of the phylum cytophaga-flavobacter-bacterioides in the natural environment. Microbiology
: 1097–1106.PubMedCrossRefGoogle Scholar
Porter KG, Feig YS. The use of DAPI for identifying and counting aquatic microflora. Limnol. Oceanogr.
: 943–948.CrossRefGoogle Scholar
Verdonck L, Swings J, Kersters K, Dehasque M, Sorgeloos P, Leger P. Variability of the microbial environment of rotifer Brachionus plicatilis
production systems. J. World Aquaculture Soc.
: 55–59.CrossRefGoogle Scholar
Verdonck L, Grisez L, Sweetmann E, Minkoff G, Sorgeloos P, Ollevier F, Swings J. Vibrios associated with routine productions of Brachionus plicatilis
: 203–214.CrossRefGoogle Scholar
Eddy SD, Jones SH. Microbiology of summer flounder Paralichthys dentatus
fingerling production at a marine fish hatchery. Aquaculture
: 9–28.CrossRefGoogle Scholar
Grisez L, Reyniers J, Verdonck L, Swings J, Ollevier F. Dominant intestinal microflora of sea bream and sea bass larvae, from two hatcheries, during larval development. Aquaculture
: 387–399.CrossRefGoogle Scholar
Pedersen K, Dalsgaard I, Larsen JL. Vibrio damsela
associated with diseased fish in Denmark. Appl. Environ. Microbiol.
: 3711–3715.PubMedGoogle Scholar
Balebona MC, Andreu MJ, Bordas MA, Zorrilla I, Morinigo MA, Borrego JJ. Pathogenicity of Vibrio alginolyticus
for cultured gilt-head sea bream (Sparus aurata
L.). Appl. Environ. Microbiol.
: 4269–4275.PubMedGoogle Scholar
Fouz B, Alcaide E, Barrera R, Amaro C. Susceptibility of Nile tilapia (Oreochromis niloticus
) to vibriosis due to Vibrio vulnificus
biotype 2 (serovar E). Aquaculture
: 21–30.CrossRefGoogle Scholar
Eilers H, Pernthaler J, Glöckner FO, Amann R. Culturability and in situ abundance of pelagic bacteria from the North Sea. Appl. Environ. Microbiol.
: 3044–3051.CrossRefPubMedGoogle Scholar
Yokokawa T, Nagata T, Cottrell MT, Kirchman DL. Growth rate of the major phylogenetic bacterial groups in the Delaware estuary. Limnol. Oceanogr.
: 1620–1629.Google Scholar
Nicolas J-L, Corre S, Cochard J-C. Bacterial population association with phytoplankton cultured in a bivalve hatchery. Microb. Ecol.
: 400–413.CrossRefPubMedGoogle Scholar
Grossart H-P, Levold F, Allgaier M, Simon M, Brinkhoff T. Marine diatom species harbour distinct bacterial communities. Environ. Microbiol.
: 860–873.CrossRefPubMedGoogle Scholar
Jasti S, Sieracki ME, Poulton NJ, Giewat MW, Rooney-Varga JN. Phylogenetic diversity and specificity of bacteria closely associated with Alexandrium
spp. and other phytoplankton. Appl. Environ. Microbiol.
: 3483–3494.CrossRefPubMedGoogle Scholar
Nakase G, Eguchi M. Analysis of bacterial communities in Nannochloropsis
sp. cultures used for larval fish production. Fish. Sci.
: 543–549.CrossRefGoogle Scholar
Cottrell MT, Kirchman D. Natural assemblages of marine proteobacteria and members of the Cytophaga-Flavobacter
cluster consuming low- and high- molecular-weight dissolved organic matter. Appl. Environ. Microbiol.
: 1692–1697.CrossRefPubMedGoogle Scholar
Waite AM, Olson RJ, Dam HG, Passow U. Sugar-containing compounds on the cell surfaces of marine diatoms measured using concanavalin A and flow cytometry. J. Phycol.
: 925–933.CrossRefGoogle Scholar
Zubkov MV, Fuchs BM, Archer SD, Kiene RP, Amann R, Burkill PH. Linking the composition of bacterioplankton to rapid turnover of dissolved dimethylsulphoniopropionate in an algal bloom in the North Sea. Environ. Microbiol.
: 304–311.CrossRefPubMedGoogle Scholar
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