Planctomycetes dominate biofilms on surfaces of the kelp Laminaria hyperborea
© Bengtsson and Øvreås; licensee BioMed Central Ltd. 2010
Received: 4 June 2010
Accepted: 15 October 2010
Published: 15 October 2010
Bacteria belonging to Planctomycetes display several unique morphological and genetic features and are found in a wide variety of habitats on earth. Their ecological roles in these habitats are still poorly understood. Planctomycetes have previously been detected throughout the year on surfaces of the kelp Laminaria hyperborea from southwestern Norway. We aimed to make a detailed investigation of the abundance and phylogenetic diversity of planctomycetes inhabiting these kelp surfaces.
Planctomycetes accounted for 51-53% of the bacterial biofilm cells in July and September and 24% in February according to fluorescence in situ hybridization (FISH) results. Several separate planctomycetes lineages within Pirellulae, Planctomyces and OM190 were represented in 16S rRNA gene clone libraries and the most abundant clones belonged to yet uncultured lineages. In contrast to the abundance, the diversity of the planctomycete populations increased from July to February and was probably influenced by the aging of the kelp tissue. One planctomycete strain that was closely related to Rhodopirellula baltica was isolated using selective cultivation techniques.
Biofilms on surfaces of L. hyperborea display an even higher proportion of planctomycetes compared to other investigated planctomycete-rich habitats such as open water, sandy sediments and peat bogs. The findings agree well with the hypothesis of the role of planctomycetes as degraders of sulfated polymeric carbon in the marine environment as kelps produce such substances. In addition, the abundant planctomycete populations on kelp surfaces and in association with other eukaryotes suggest that coexistence with eukaryotes may be a key feature of many planctomycete lifestyles.
Bacteria belonging to the phylum Planctomycetes have revealed several remarkable features that set them apart from other bacteria. Their cryptic morphology led early microbiologists to mistake them for fungi, and the discovery of their cell compartmentalization, featuring membrane bounded organelles, raised fundamental questions about the evolution of eukaryotes [1, 2]. Further, the unique anammox metabolism found in some planctomycetes has revolutionized the view of microbial nitrogen cycling . The planctomycetes also possess cell walls without peptidoglycan, a characteristic that they share only with the obligate intracellular bacteria within Chlamydiae. In addition to the interest sparked by these unusual and fascinating features, planctomycetes have in later years attracted considerable attention because of their presence in a wide variety of environments on earth. By investigating bacterial communities using molecular methods (sequences coding for 16S rRNA), planctomycetes have been repeatedly detected in soil, sediments, marine and freshwater systems and in terrestrial hot springs to mention just a few (for a detailed review see ). However, their metabolic potential and function in these ecosystems is often unclear, as 16S rRNA gene sequence investigations only rarely give clues to ecological roles.
In the marine environment, DeLong and co-workers  found that planctomycetes were more abundant in clone libraries from marine aggregate (marine snow) attached bacteria than from free-living bacteria. Since then, results from several studies suggest that planctomycetes favor a biofilm lifestyle, adhering to surfaces in aquatic environments including marine sediments  (among others), diatom cells , seaweeds and other aquatic macrophytes [8, 9]. Rhodopirellula baltica is an extensively studied marine particle-attached planctomycete. Its genome sequence reveals a large number of genes involved in the breakdown of sulfated polysaccharides , a carbon source found in marine photosynthetic organisms such as microalgae and seaweeds, who's detrital material is thought to generate marine snow. Such genes are also encountered in other planctomycete genomes and planctomycete-derived metagenomic fosmid libraries from seawater collected in upwelling zones . The overrepresentation of such genes, and the association of R. baltica and other planctomycetes with marine snow has led to the hypothesis that heterotrophic planctomycetes are specialized degraders of sulfated polymeric carbon, for example in marine snow [10, 11]. Given the significance of marine snow as part of the so-called "biological pump" of carbon in the oceans [12, 13], planctomycetes may thereby be playing a crucial role in global carbon turnover . Still, quantitative data on the distribution of planctomycetes in the marine environment and elsewhere is still scarce, and very little is known about the yet uncultured planctomycete lineages that are assumed to carry out the bulk of these globally critical processes.
Kelps are large brown seaweeds of the order Laminariales. They often form dense stands along rocky coastlines that are referred to as kelp forests. Kelp forest ecosystems are some of the most productive ecosystems in the world . Their immense importance for coastal biodiversity, productivity and human economy has long been recognized in temperate regions of the world and is only beginning to be understood in the tropics . Kelp forests along the Atlantic coasts of Europe are dominated by the large kelp Laminaria hyperborea. Bacteria associated to kelp are believed to be important in the carbon and nitrogen turnover in kelp forest food webs [16, 17], but it is still not known what types of bacteria are involved in these processes. Recently, the seasonal dynamics of the cell density and bacterial community composition in biofilms on L. hyperborea were addressed. In this study, planctomycetes were frequently detected throughout the year but their abundance and phylogenetic relationships were not considered . In order to address the importance of this group of bacteria in kelp forests, we therefore aimed to take an in-depth look at the abundance and phylogenetic diversity of planctomycete communities inhabiting L. hyperborea surface biofilms. This was achieved by using fluorescence in situ hybridization (FISH) to quantify their abundance and visualize their distribution in the biofilm as well as 16S rRNA gene clone library construction to elucidate their phylogenetic relationships, community composition and diversity at different times of the year. In addition, a selective cultivation approach was used to assess the culturability of planctomycetes from kelp surfaces.
Abundance of planctomycetes in kelp surface biofilms
A summary of the results
Avg. cells/cm2 (DAPI) ± 1SD
Avg.% Eub338 I-III of DAPI ± 1SD
Avg.% Pla46 of DAPI ± 1SD
% Pla46 of Eub338 I-III
No. of clones
No. of OTUs (98%)
Shannon diversity index
Chao1 OTU richness estimate ± SE
8.2e+06 ± 1.9e+06
51.6 ± 18.5
23.7 ± 9.3
29 ± 12.5
7.4e+06 ± 4.8e+06
78.7 ± 5.2
52.5 ± 9.3
9 ± 0.73
1.7e+07 ± 6.4e+06
73.6 ± 4.7
50.8 ± 7.2
16 ± 3.4
Cell distribution of planctomycetes in the biofilms
Isolation and cultivation of planctomycetes from kelp surfaces
Phylogenetic diversity of planctomycetes from kelp surface biofilms
Three clone libraries, from February 2007, July 2007 and September 2008, constructed with the Planctomycetes-specific primer Pla46f and the general bacterial primer 1542r were analyzed to gain insight into the phylogenetic diversity of the planctomycetes growing in kelp surface biofilms. In total, 266 clones were sequenced in the forward direction from the three clone libraries, resulting in partial 16S rRNA gene sequences of approximately 850 basepairs. Of these, only 9 sequences (3.4%) did not classify as belonging to Planctomycetes and were discarded from the further analyses. These unspecific sequences classified as Deltaproteobacteria (three), Gammaproteobacteria (two), Actinobacteria (two) and Verrucomicrobia (one) while one remained unclassified using the Greengenes G2Chip classifier . The remaining 257 partial planctomycete 16S rRNA gene sequences clustered into 23 OTUs at 98% sequence similarity. Other OTU definitions (95-99%) gave different numbers of OTUs, but the general trends observed in the dataset were the same. One to six representative clones of each OTU were selected for sequencing in the reverse direction in order to assemble near full-length 16S rRNA gene sequences. Of the assembled sequences, three were removed from the analyses because of poor sequence quality and two because of indications of chimeric origin. The remaining 46 near full-length planctomycete 16S rRNA gene sequences have been deposited to GenBank under the accession numbers HM369064 to HM369109, and the sequence of the P1 isolate under HM369063.
The phylogenetic analysis of the near full-length sequences obtained in this study and other planctomycete sequences obtained from the Silva reference database  revealed that highly divergent lineages of the Planctomycetes phylum are represented in kelp surface biofilms (Figure 4). The kelp surface biofilm clone sequences appear to cluster within five major lineages that have been labeled as: "RB1" and "RB2" (defined in this study), Rhodopirellula, Planctomyces and "OM190". The "RB1" and "RB2" lineages appear more closely related to the Rhodopirellula and Blastopirellula genera than to the Pirellula genus and were given their labels based on that (RB = Rhodopirellula/Blastopirellula). Yet the phylogenetic analyses do not place them consistently with either of the genera. Sequence similarities of 86-90% to Rhodopirellula baltica and Blastopirellula marina indicate that they probably represent distinct phylogenetic lineages that could correspond to new genera according to conventional taxonomical practice. The "RB1" lineage was by far the most represented in all three clone libraries (Figure 4). Sequences that cluster within the "RB2", Rhodopirellula and Planctomyces lineages were only represented in September and February, indicating a seasonal difference, while OM190 representatives were present at low numbers in all three clone libraries (Figure 4).
To our knowledge, the kelp surface biofilms investigated in this study display the highest proportion of bacteria belonging to Planctomycetes reported in a natural bacterial community so far. This observation is consistent with earlier results from a DGGE based study on seasonal variation of Laminaria hyperborea (kelp) surface biofilm communities . Other habitats where a high abundance of planctomycetes has been reported include seawater during a diatom bloom where planctomycetes related to Pirellula were detected attached to diatom cells and were among the dominant lineages in the bloom samples . In investigations of sandy sediments containing algal cells [24, 25], planctomycetes were also abundant, accounting for up to 20% of total cells, accompanied by Cytophaga/Flavobacteria. Gade and co-workers  used order-, genus- and strain specific FISH probes to detect planctomycetes in a range of aquatic habitats and recorded abundances up to 11% of total cells in some lakes. Peat bogs with Sphagnum moss have also been reported to harbor abundant (up to 13% of total bacterial numbers) planctomycete populations . Similarly to kelp surfaces, these environments are all highly influenced by photosynthetic eukaryotes.
The studies mentioned above have all quantified planctomycetes using specific FISH probes. Several other studies have detected planctomycetes using PCR based cloning and fingerprinting methods followed by sequencing. Two of the most frequently used general bacterial PCR primers, targeting the 16S rRNA gene around E. coli positions 8-27 and 338-355, contain mismatches against planctomycete sequences [27, 28]. This may have caused planctomycete abundances to be underestimated in many habitats, leading investigators to turn their attention towards bacterial groups that appear more abundant. Despite awareness of this problem, the literature and the sequence databases probably reflect a tradition of neglect towards the planctomycetes. In the light of this, it is difficult to say whether the dominance of planctomycetes on Laminaria hyperborea surface biofilms represents a unique feature of this habitat, or if other planctomycete-dominated bacterial communities have been overlooked until now. For example, Staufenberger and co-workers  did not detect planctomycetes in surface biofilms of another species of kelp (Saccharina latissima) using general bacterial primers for cloning and DGGE analysis. Yet, use of different primers has let to the detection of planctomycetes on both the kelps S. latissima and Laminaria digitata (Bengtsson, unpublished results).
A possible explanation for the suitability of kelp as a habitat for planctomycetes is its content of sulfated polysaccharides, a class of molecules that some marine planctomycetes are known for being able to degrade . For example, Laminaria hyperborea contains fucoidan, a class of complex brown algal sulfated polysaccharides. These substances are secreted to the surface of L. hyperborea via mucilage channels . It is reasonable to assume that planctomycetes living on kelp surfaces utilize substances produced by the kelp, for example fucoidan, as carbon sources. However, the presence of suitable carbon sources appears insufficient to explain the observed dominance of planctomycetes, as they must not only be able to grow and divide, but also outcompete other bacteria to be successful. Another contributing factor to the success of planctomycetes on kelp surfaces may be resistance to chemical antimicrobial defense compounds produced by the kelp. Antibacterial activity has been detected in extracts from many species of kelp, yet the substances responsible for the activity have often not been identified . The lack of peptidoglycan in planctomycete cell walls makes them resistant to conventional cell wall targeting antibiotics like ampicillin. Resistance to other antibiotics, targeting for example protein synthesis (streptomycin) has also been reported in some marine planctomycetes [32, 33].
In many cases the reference sequences that are the most closely related to kelp surface planctomycetes are obtained from other marine eukaryotes such as for example red and green seaweeds, corals, crustaceans and sponges (Figure 4). The frequent association of planctomycetes to eukaryotes has previously been noted . This could point to a general lifestyle pattern of heterotrophic planctomycetes. They may combine an affinity for sulfated polysaccharides and other polymeric carbon molecules [10, 11] produced by their eukaryote hosts with a resistance to eukaryote chemical defense molecules. The resulting competitive advantage over other bacterial groups that are utilizing the same kind of substrates, for example the Bacteroidetes  might be one of the keys to the success of planctomycetes in a wide variety of environments on earth.
Our results show differences between the different sampling times (February, July and September), in planctomycete abundance, OTU composition and diversity. For example, in February there is a relatively low abundance of planctomycetes (Figure 1) compared to July and September. This may be linked to the age of the kelp tissue, as the kelp lamina is older in February compared to in July and September due to the seasonal growth cycle of the kelp. Aging of the kelp tissue could be associated with lowered antibacterial chemical defense by the kelp, as the old kelp lamina is to be shed soon after February, and does therefore not need to be defended against microbial colonization. Without the presence of chemical defense substances, the planctomycetes could loose their competitive advantage over other bacterial groups, explaining their lower abundance in February. The senescence of the kelp tissue as it ages could also cause the appearance of new niches involved in degradation of different kelp constituents, thereby enabling the more diverse planctomycete communities that are observed in February compared to July and September (Table 1, Figure 6).
Among the different planctomycete lineages that are represented on the kelp, the lineage defined as "RB1" in this study appears to be the most abundant, accounting for a majority of the clones at all sampling times (Figure 4). The high abundance of RB1 planctomycetes may thus be the cause of the observed dominance of planctomycetes on kelp surfaces (Figs. 1 and 2). Their high abundance implies a lifestyle that makes them particularly successful on kelp surfaces. Yet the lineage also includes reference sequences from a variety of other marine habitats, indicating that RB1 is not a kelp-specific lineage. The RB1 and RB2 lineages, defined in this study, are clearly related to the "Pirellulae", a lineage including the genera Pirellula, Rhodopirellula and Blastopirellula (formerly all included in the genus Pirellula). Yet our phylogenetic analyses did not place them reliably with any of the described genera, indicated by the bootstrap support for the relevant branches in Figure 4. There are no sequences of cultured strains within the RB1 and RB2 lineages available in the databases. Another uncultured lineage, the so-called OM190 planctomycetes (Silva taxonomy) is also represented by clones from kelp surfaces at all sampling times, yet in low numbers. This is a lineage that appears to branch off deeply in the planctomycete tree and representatives have been detected in a variety of environments including seawater , soil  and marine eukaryotes [8, 38]. These lineages have yet to be cultured and described and will reveal valuable information on planctomycete metabolism and evolution if cultivation is successful.
Using conventional approaches, the Rhodopirellula sp. strain P1 could easily be isolated. Several closely related strains have been brought into culture earlier . However, the 16S rRNA gene sequence of P1 does not correspond to any of the abundant OTUs detected on the kelp surfaces, for example within the RB1 lineage. Kelp surfaces are nevertheless a promising source for isolation of novel planctomycete strains, using more ambitious and creative approaches that take into account the environmental factors experienced by bacteria on kelp surfaces. The rewards awaiting such attempts can be substantial, given the representation of highly divergent lineages of the planctomycete tree in kelp surface biofilms.
Kelp (Laminaria hyperborea) surface biofilms have a uniquely high relative abundance of planctomycetes. Several distinct lineages are represented, and the diversity and composition of the planctomycetes change during the year, probably influenced by aging of the kelp tissue. The finding of abundant planctomycete populations in kelp surface biofilms agrees well with the view of heterotrophic planctomycetes as surface attached, specialized degraders of sulfated polysaccharides in the marine environment, as kelps are known to produce such substances. Furthermore, we wish to extend this view by hypothesizing that many heterotrophic planctomycetes share a preference of intimate coexistence with eukaryotes, which may be linked to antibiotic resistance. The study addresses the urgent need for more detailed, quantitative knowledge on the diverse marine planctomycetes.
Sample collection and preparation
Kelp (Laminaria hyperborea) was collected at one site near Bergen, Norway (60° 09.706' N, 5° 02.371' E) in February 2007 and in July 2007. These sampling times were selected based on a previous study that detected low (February) and high proportions (July) of planctomycetes at these times . In addition, kelp was sampled at the same site in September 2008 to obtain fresh biofilm material for cultivation of planctomycetes. Six replicate kelp individuals were collected from a depth of 5 to 9 m by dredging from a boat at each sampling occasion and were kept cool until further processing (a few hours). Biofilm samples were obtained from the middle part of the kelp lamina (blade) of each kelp individual. The lamina areas used for biofilm sampling were thoroughly washed with sterile seawater. Biofilm for DNA extraction was sampled by scraping off material from the kelp surface with a sterile scalpel as described previously . Biofilm for FISH was sampled by cutting out whole pieces of the kelp lamina in order for the attached biofilm to remain intact. Sample collection and preparation procedures are described in greater detail in .
Kelp lamina pieces (1 × 0.5 cm) were fixed in 2% buffered paraformaldehyde overnight, washed twice in 50% EtOH in PBS and stored in the same solution at -20°C. Prior to FISH, the kelp pieces were dehydrated in 96% EtOH and air-dried. Each sample kelp piece was further divided into 0.5 × 0.5 cm pieces, that were used for hybridization either with the general Bacterial probe mix Eub338 I-III  or the planctomycete specific probe Pla46 . In addition, a subset of samples were hybridized with the probe Pir1223  that is reported to be specific for the genera Pirellula, Blastopirellula and Rhodopirellula (formerly all included in Pirellula). Several samples were also hybridized with the Non338 probe to check for signals caused by unspecific hybridization or autofluorescence of bacterial cells. All probes were bound to the fluorochrome Cy3, as previous investigations have shown that it gives superior fluorescence signals over the otherwise troublesome autofluorescence of the kelp cells compared to other fluorochromes such as fluorescein (Bengtsson, unpublished data). The formamide concentrations in the hybridization solution for the respective probes were 35% for the Eub338 I-III mix, 30% for Pla46 and 30% for Pir1223. Formamide concentrations of 20, 25, 30, 35 and 40% were evaluated on a subset of the September samples for the Pla46 probe. FISH was carried out according to  with some modifications. In summary, the dry kelp pieces were soaked in hybridization solution and hybridized at 46°C for 3 hours inside capped 0.5 ml plastic tubes. After stringent washing and subsequent washing with dH2O, the kelp pieces were counter-stained with DAPI and mounted on glass slides as described in .
Digital images of randomly selected microscopic fields were captured for counting of DAPI stained cells and FISH hybridized cells. Image capture and counting were carried out as previously described . The percentage FISH hybridized cells of the total cell count (DAPI stained cells) was calculated for every individual microscope field captured, and an average percentage was calculated for each sample.
Isolation and cultivation of planctomycetes from kelp surfaces
Freshly scraped off biofilm material from September 2008 suspended in sterile seawater was used to inoculate M30 medium  diluted in 3/4 parts sterile seawater supplemented with ampicillin (0.2 mg/ml). After growth was detected, the liquid culture was plated out on M30 medium solidified with gellan gum (Gelzan, Sigma-Aldrich), and individual colonies were picked and re-plated several times to obtain pure cultures.
Scraped off biofilm was suspended in sterile filtered and autoclaved seawater and the cells were pelleted by centrifugation. DNA was extracted from the pellets as previously described . Equal volumes of the DNA extracts from the 6 replicate kelp plants from each sampling time were pooled into one sample per sampling time. The purpose if this was to obtain an overall picture of the planctomycete populations at each sampling time. Variation in OTU composition between individual kelp laminae is not captured by this approach, but has been addressed previously for the whole bacterial communities . The pooled DNA extracts (from February 2007, July 2007 and September 2008) were used for the subsequent PCR amplification and clone library construction.
PCR amplification and clone library construction
The Planctomycetes specific forward primer Pla46f (5'-GGA TTA GGC ATG CAA GTC-3') complementary to the Pla46 FISH probe  and the general bacterial reverse primer 1542r (5'-AAG GAG GTG ATC CAG CCG CA-3')  were used to amplify a near full length fragment of the 16S rRNA gene of Planctomycetes. PCR conditions were: 94°C for 5 min, 25 cycles of 94°C for 1 min, 60°C for 1 min, 72°C for 2 min, and final elongation at 72°C for 10 min. Each 25 μl PCR reaction contained nuclease-free water, F511 buffer (Finnzymes), 0.1 mM of each dNTP (F506L, Finnzymes), 0.02% BSA, 0.5 μM of each primer, 0.02 U Dynazyme II F501-L (Finnzymes), and approximately 30 ng template DNA. Three clone libraries, one from each sampling occasion, were constructed using the TOPO TA cloning kit (Invitrogen). Ninety-six clones were picked from each clone library. Cloned fragments were reamplified using the supplied M13 primer pair according to the manufacturers instructions.
Sequencing and sequence processing
All cloned fragments were sequenced in one direction using the Pla46f primer. Sequencing was carried out with the BigDye Terminator v3.1 kit (Applied Biosystems) at the Bergen Sequencing Facility http://www.seqlab.uib.no using an ABI 3700 sequencing system. Base calling from the chromatogram files was done using the Phred software  (version 0.020425.c). The resulting sequences representing partial fragments of the 16S rRNA gene were used to select a subset of clones to sequence in the reverse direction in order to obtain near complete length 16S rRNA gene fragments. The sequences were trimmed to approximately 750 bp of good quality sequence and aligned against the Silva seed alignment (release 102) using the SINA web aligner . The alignment was imported into the ARB software package  (version 5.0) and was manually edited to improve alignment quality. The resulting alignment was used to create a distance matrix in ARB, which was used to cluster the sequences into OTUs using the furthest neighbor algorithm in the Mothur software  (version 1.9.0). Rarefaction and overlap analysis were carried out in Mothur. The Shannon diversity index and the Chao1 richness estimate was calculated in the R statistical environment (, functions: diversity and estimateR, package: vegan). Based on the OTU clustering, one to six representatives of each OTU were sequenced in reverse using the 1542r primer. The resulting sequences were assembled using CAP3  with the corresponding forward sequences to build contigs spanning nearly the full length of the 16S rRNA gene. The contigs were manually cropped to roughly the same length using the Phred base quality scores of the ends of the contigs as a guide. The resulting same-length (about 1250 bp), good quality contiguous sequences were checked for chimeras using Bellerophon  through the online Greengenes interface . The Rhodopirellula sp. strain P1 was sequenced in forward and reverse direction several times with different 16S rRNA gene primers. The individual sequence reads were manually assembled into one full-length consensus sequence.
Phylogenetic tree reconstruction
The near full-length sequences were aligned using the SINA web aligner, imported into ARB and edited as described in the previous section. Reference sequences that were closely related to the clone sequences from this study and sequences from cultured planctomycetes were selected from the SILVA database and were included in the tree calculations. Several tree calculation methods including neighbor joining (NJ), maximum likelihood (ML) and maximum parsimony (MP) were used in combination with different conservatory filters in ARB and the tree topologies compared to ensure a reliable result. The final ML tree was calculated in ARB with 175 sequences using PhyML  applying bootstrap analysis (1000 bootstraps) and no filter. Four Verrucomicrobia sequences (accession numbers: AY271254, DQ302104, AB297805, AB297806) were used as an outgroup in the tree calculation. The tree was edited by removing some of the reference sequences for clarity of presentation and the final result is shown in Figure 4.
The authors wish to thank Tomas Sørlie and Julia Storesund for sampling assistance, Friederike Hoffmann for valuable advice on FISH and Anders Lanzén for bioinformatics assistance. Kjersti Sjøtun, Antonio García Moyano, Jeffrey Keen, Tim Urich and three anonymous reviewers provided constructive comments that considerably improved the manuscript. Funding for sampling and laboratory expenses was provided by FMC Biopolymer. The authors are funded by the University of Bergen.
- Lindsay MR, Webb RI, Strous M, Jetten MS, Butler MK, Forde RJ, Fuerst JA: Cell compartmentalisation in planctomycetes: novel types of structural organisation for the bacterial cell. Arch Microbiol. 2001, 175 (6): 413-429. 10.1007/s002030100280.View ArticlePubMedGoogle Scholar
- Fuerst JA: Intracellular compartmentation in planctomycetes. Annual review of microbiology. 2005, 59: 299-328. 10.1146/annurev.micro.59.030804.121258.View ArticlePubMedGoogle Scholar
- Strous M, Fuerst JA, Kramer EHM, Logemann S, Muyzer G, van de Pas-Schoonen KT, Webb R, Kuenen JG, Jetten MSM: Missing lithotroph identified as new planctomycete. Nature. 1999, 400 (6743): 446-449. 10.1038/22749.View ArticlePubMedGoogle Scholar
- Ward N, Staley JT, Fuerst JA, Giovannoni S, Schlesner H, Stackebrandt E: The Order Planctomycetales, Including the Genera Planctomyces, Pirellula, Gemmata and Isosphaera and the Candidatus Genera Brocadia, Kuenenia and Scalindua. The Prokaryotes. 2006, New York: Springer, 7: 3Google Scholar
- Delong EF, Franks DG, Alldredge AL: Phylogenetic diversity of aggregate-attached vs. free-living marine bacterial assemblages. Limnol Oceanogr. 1993, 38 (5): 924-934. 10.4319/lo.1993.38.5.0924.View ArticleGoogle Scholar
- Gray JP, Herwig RP: Phylogenetic analysis of the bacterial communities in marine sediments. Applied and Environmental Microbiology. 1996, 62 (11): 4049-4059.PubMed CentralPubMedGoogle Scholar
- Morris RM, Longnecker K, Giovannoni SJ: Pirellula and OM43 are among the dominant lineages identified in an Oregon coast diatom bloom. Environmental Microbiology. 2006, 8 (8): 1361-1370. 10.1111/j.1462-2920.2006.01029.x.View ArticlePubMedGoogle Scholar
- Longford SR, Tujula NA, Crocetti GR, Holmes AJ, Holmstroem C, Kjelleberg S, Steinberg PD, Taylor MW: Comparisons of diversity of bacterial communities associated with three sessile marine eukaryotes. Aquat Microb Ecol. 2007, 48: 217-229. 10.3354/ame048217.View ArticleGoogle Scholar
- Hempel M, Blume M, Blindow I, Gross EM: Epiphytic bacterial community composition on two common submerged macrophytes in brackish water and freshwater. Bmc Microbiol. 2008, 8: 58-10.1186/1471-2180-8-58.PubMed CentralView ArticlePubMedGoogle Scholar
- Glöckner FO, Kube M, Bauer M, Teeling H, Lombardot T, Ludwig W, Gade D, Beck A, Borzym K, Heitmann K, et al: Complete genome sequence of the marine planctomycete Pirellula sp. strain 1. Proc Natl Acad Sci USA. 2003, 100 (14): 8298-8303. 10.1073/pnas.1431443100.PubMed CentralView ArticlePubMedGoogle Scholar
- Woebken D, Teeling H, Wecker P, Dumitriu A, Kostadinov I, DeLong EF, Amann R, Gloeckner FO: Fosmids of novel marine Planctomycetes from the Namibian and Oregon coast upwelling systems and their cross-comparison with planctomycete genomes. ISME J. 2007, 1 (5): 419-435. 10.1038/ismej.2007.63.View ArticlePubMedGoogle Scholar
- Shanks AL, Trent JD: Marine snow - sinking rates and potential role in vertical flux. Deep-Sea Res. 1980, 27 (2): 137-143. 10.1016/0198-0149(80)90092-8.View ArticleGoogle Scholar
- Longhurst AR: Role of the marine biosphere in the global carbon cycle. Limnol Oceanogr. 1991, 36 (8): 1507-1526. 10.4319/lo.19220.127.116.117.View ArticleGoogle Scholar
- Mann KH: Seaweeds - their productivity and strategy for growth. Science. 1973, 182 (4116): 975-981. 10.1126/science.182.4116.975.View ArticlePubMedGoogle Scholar
- Graham MH, Kinlan BP, Druehl LD, Garske LE, Banks S: Deep-water kelp refugia as potential hotspots of tropical marine diversity and productivity. Proc Natl Acad Sci USA. 2007, 104 (42): 16576-16580. 10.1073/pnas.0704778104.PubMed CentralView ArticlePubMedGoogle Scholar
- Norderhaug KM, Nygaard K, Fredriksen S: Trophic importance of Laminaria hyperborea to kelp forest consumers and the importance of bacterial degradation to food quality. Marine Ecology Progress Series. 2003, 255: 135-144. 10.3354/meps255135.View ArticleGoogle Scholar
- Newell RC, Field JG: The contribution of bacteria and detritus to carbon and nitrogen flow in a benthic community. Marine Biology Letters. 1983, 4 (1): 23-36.Google Scholar
- Bengtsson MM, Sjøtun K, Øvreås L: Seasonal dynamics of bacterial biofilms on the kelp Laminaria hyperborea. Aquat Microb Ecol. 2010, 60: 71-83. 10.3354/ame01409.View ArticleGoogle Scholar
- Neef A, Amann R, Schlesner H, Schleifer KH: Monitoring a widespread bacterial group: in situ detection of planctomycetes with 16S rRNA-targeted probes. Microbiol-Uk. 1998, 144: 3257-3266. 10.1099/00221287-144-12-3257.View ArticleGoogle Scholar
- Gade D, Schlesner H, Glockner FO, Amann R, Pfeiffer S, Thomm A: Identification of planctomycetes with order-, genus-, and strain-specific 16S rRNA-targeted probes. Microbial Ecology. 2004, 47 (3): 243-251. 10.1007/s00248-003-1016-9.View ArticlePubMedGoogle Scholar
- Winkelmann N, Harder J: An improved isolation method for attached-living Planctomycetes of the genus Rhodopirellula. J Microbiol Methods. 2009, 77 (3): 276-284. 10.1016/j.mimet.2009.03.002.View ArticlePubMedGoogle Scholar
- DeSantis TZ, Hugenholtz P, Larsen N, Rojas M, Brodie EL, Keller K, Huber T, Dalevi D, Hu P, Andersen GL: Greengenes, a chimera-checked 16S rRNA gene database and workbench compatible with ARB. Appl Environ Microb. 2006, 72: 5069-5072. 10.1128/AEM.03006-05.View ArticleGoogle Scholar
- Pruesse E, Quast C, Knittel K, Fuchs BM, Ludwig W, Peplies J, Gloeckner FO: SILVA: a comprehensive online resource for quality checked and aligned ribosomal RNA sequence data compatible with ARB. Nucleic Acids Res. 2007, 35: 7188-7196. 10.1093/nar/gkm864.PubMed CentralView ArticlePubMedGoogle Scholar
- Rusch A, Huettel M, Reimers CE, Taghon GL, Fuller CM: Activity and distribution of bacterial populations in Middle Atlantic Bight shelf sands. FEMS Microbiology Ecology. 2003, 44 (1): 89-100. 10.1111/j.1574-6941.2003.tb01093.x.View ArticlePubMedGoogle Scholar
- Musat N, Werner U, Knittel K, Kolb S, Dodenhof T, van Beusekom JEE, de Beer D, Dubilier N, Amann R: Microbial community structure of sandy intertidal sediments in the North Sea, Sylt-Romo Basin, Wadden Sea. Syst Appl Microbiol. 2006, 29 (4): 333-348. 10.1016/j.syapm.2005.12.006.View ArticlePubMedGoogle Scholar
- Kulichevskaya IS, Pankratov TA, Dedysh SN: Detection of representatives of the Planctomycetes in Sphagnum peat bogs by molecular and cultivation approaches. Microbiology. 2006, 75 (3): 329-335. 10.1134/S0026261706030155.View ArticleGoogle Scholar
- Vergin KL, Urbach E, Stein JL, DeLong EF, Lanoil BD, Giovannoni SJ: Screening of a fosmid library of marine environmental genomic DNA fragments reveals four clones related to members of the order Planctomycetales. Appl Environ Microbiol. 1998, 64 (8): 3075-3078.PubMed CentralPubMedGoogle Scholar
- Daims H, Brühl A, Amann R, Schleifer KH, Wagner M: The domain-specific probe EUB338 is insufficient for the detection of all Bacteria: development and evaluation of a more comprehensive probe set. Syst Appl Microbiol. 1999, 22 (3): 434-444.View ArticlePubMedGoogle Scholar
- Staufenberger T, Thiel V, Wiese J, Imhoff JF: Phylogenetic analysis of bacteria associated with Laminaria saccharina. Fems Microbiol Ecol. 2008, 64 (1): 65-77. 10.1111/j.1574-6941.2008.00445.x.View ArticlePubMedGoogle Scholar
- Evans LV, Simpson M, Callow ME: Sulphated Polysaccharide Synthesis in Brown Algae. Planta. 1973, 110: 237-252. 10.1007/BF00387636.View ArticlePubMedGoogle Scholar
- Bhadury P, Wright PC: Exploitation of marine algae: biogenic compounds for potential antifouling applications. Planta. 2004, 219 (4): 561-578. 10.1007/s00425-004-1307-5.View ArticlePubMedGoogle Scholar
- Fuerst JA, Sambhi SK, Paynter JL, Hawkins JA, Atherton JG: Isolation of a bacterium resembling Pirellula species from primary tissue culture of the giant tiger prawn (Penaeus monodon). Applied and Environmental Microbiology. 1991, 57 (11): 3127-3134.PubMed CentralPubMedGoogle Scholar
- Fuerst JA, Gwilliam HG, Lindsay M, Lichanska A, Belcher C, Vickers JE, Hugenholtz P: Isolation and molecular identification of planctomycete bacteria from postlarvae of the giant tiger prawn, Penaeus monodon. Applied and Environmental Microbiology. 1997, 63 (1): 254-262.PubMed CentralPubMedGoogle Scholar
- Wagner M, Horn M: The Planctomycetes, Verrucomicrobia, Chlamydiae and sister phyla comprise a superphylum with biotechnological and medical relevance. Current Opinion in Biotechnology. 2006, 17 (3): 241-9. 10.1016/j.copbio.2006.05.005.View ArticlePubMedGoogle Scholar
- Bauer M, Kube M, Teeling H, Richter M, Lombardot T, Allers E, Wuerdemann CA, Quast C, Kuhl H, Knaust F, et al: Whole genome analysis of the marine Bacteroidetes 'Gramella forsetii' reveals adaptations to degradation of polymeric organic matter. Environmental Microbiology. 2006, 8 (12): 2201-2213. 10.1111/j.1462-2920.2006.01152.x.View ArticlePubMedGoogle Scholar
- Rappe MS, Kemp PF, Giovannoni SJ: Phylogenetic diversity of marine coastal picoplankton 16S rRNA genes cloned from the continental shelf off Cape Hatteras, North Carolina. Limnol Oceanogr. 1997, 42 (5): 811-826. 10.4319/lo.1997.42.5.0811.View ArticleGoogle Scholar
- Elshahed MS, Youssef NH, Spain AM, Sheik C, Najar FZ, Sukharnikov LO, Roe BA, Davis JP, Schloss PD, Bailey VL, et al: Novelty and uniqueness patterns of rare members of the soil biosphere. Appl Environ Microb. 2008, 74 (17): 5422-5428. 10.1128/AEM.00410-08.View ArticleGoogle Scholar
- Mohamed NM, Saito K, Tal Y, Hill RT: Diversity of aerobic and anaerobic ammonia-oxidizing bacteria in marine sponges. Isme J. 2010, 4 (1): 38-48. 10.1038/ismej.2009.84.View ArticlePubMedGoogle Scholar
- Glöckner FO, Amann R, Alfreider A, Pernthaler J, Psenner R, Trebesius K, Schleifer KH: An in situ hybridization protocol for detection and identification of planktonic bacteria. Syst Appl Microbiol. 1996, 19 (3): 403-406.View ArticleGoogle Scholar
- Edwards U, Rogall T, Blöcker H, Emde M, Böttger EC: Isolation and direct complete nucleotide determination of entire genes. Characterization of a gene coding for 16S ribosomal RNA. Nucleic Acids Res. 1989, 17 (19): 7843-7853. 10.1093/nar/17.19.7843.PubMed CentralView ArticlePubMedGoogle Scholar
- Ewing B, Hillier L, Wendl MC, Green P: Base-calling of automated sequencer traces using phred. I. Accuracy assessment. Genome Res. 1998, 8 (3): 175-185.View ArticlePubMedGoogle Scholar
- Ludwig W, Strunk O, Westram R, Richter L, Meier H, Yadhukumar , Buchner A, Lai T, Steppi S, Jobb G, et al: ARB: a software environment for sequence data. Nucleic Acids Res. 2004, 32 (4): 1363-1371. 10.1093/nar/gkh293.PubMed CentralView ArticlePubMedGoogle Scholar
- Schloss PD, Westcott SL, Ryabin T, Hall JR, Hartmann M, Hollister EB, Lesniewski RA, Oakley BB, Parks DH, Robinson CJ, et al: Introducing mothur: Open-Source, Platform-Independent, Community-Supported Software for Describing and Comparing Microbial Communities. Applied and Environmental Microbiology. 2009, 75 (23): 7537-7541. 10.1128/AEM.01541-09.PubMed CentralView ArticlePubMedGoogle Scholar
- R Development Core Team: R: A language and environment for statistical computing. R Foundation for Statistical Computing, Vienna, Austria ISBN 3-900051-07-0. 2009,http://www.R-project.orgGoogle Scholar
- Huang XQ, Madan A: CAP3: A DNA sequence assembly program. Genome Res. 1999, 9 (9): 868-877. 10.1101/gr.9.9.868.PubMed CentralView ArticlePubMedGoogle Scholar
- Huber T, Faulkner G, Hugenholtz P: Bellerophon: a program to detect chimeric sequences in multiple sequence alignments. Bioinformatics. 2004, 20 (14): 2317-2319. 10.1093/bioinformatics/bth226.View ArticlePubMedGoogle Scholar
- Guindon S, Gascuel O: A simple, fast, and accurate algorithm to estimate large phylogenies by maximum likelihood. Syst Biol. 2003, 52 (5): 696-704. 10.1080/10635150390235520.View ArticlePubMedGoogle Scholar
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