A novel uncultured heterotrophic bacterial associate of the cyanobacterium Moorea producens JHB
- Susie L. Cummings†1, 2,
- Debby Barbé†2,
- Tiago Ferreira Leao†2,
- Anton Korobeynikov3, 4,
- Niclas Engene5,
- Evgenia Glukhov2,
- William H. Gerwick2, 6 and
- Lena Gerwick2Email author
© The Author(s). 2016
Received: 27 June 2015
Accepted: 19 August 2016
Published: 30 August 2016
Filamentous tropical marine cyanobacteria such as Moorea producens strain JHB possess a rich community of heterotrophic bacteria on their polysaccharide sheaths; however, these bacterial communities have not yet been adequately studied or characterized.
Results and discussion
Through efforts to sequence the genome of this cyanobacterial strain, the 5.99 MB genome of an unknown bacterium emerged from the metagenomic information, named here as Mor1. Analysis of its genome revealed that the bacterium is heterotrophic and belongs to the phylum Acidobacteria, subgroup 22; however, it is only 85 % identical to the nearest cultured representative. Comparative genomics further revealed that Mor1 has a large number of genes involved in transcriptional regulation, is completely devoid of transposases, is not able to synthesize the full complement of proteogenic amino acids and appears to lack genes for nitrate uptake. Mor1 was found to be present in lab cultures of M. producens collected from various locations, but not other cyanobacterial species. Diverse efforts failed to culture the bacterium separately from filaments of M. producens JHB. Additionally, a co-culturing experiment between M. producens JHB possessing Mor1 and cultures of other genera of cyanobacteria indicated that the bacterium was not transferable.
The data presented support a specific relationship between this novel uncultured bacterium and M. producens, however, verification of this proposed relationship cannot be done until the “uncultured” bacterium can be cultured.
Filamentous cyanobacteria, bathed in seawater and often growing in nutrient-rich environments, are surrounded by diverse communities of heterotrophic bacteria. The heterotrophic bacteria closely associated with cyanobacteria likely consume released nutrients, but may also produce vitamins and other factors useful to cyanobacterial growth, as well as assisting in cycling of CO2 and phosphate, or lowering O2 levels for oxygen-sensitive processes such as nitrogen fixation [1, 2]. Various studies have classified some of the taxa of heterotrophic bacteria that live in close proximity to cyanobacterial blooms, including common aquatic phyla such as Proteobacteria, Bacteroidetes, Actinobacteria, and Planctomycetes [3, 4]. Some potentially new species or genera were also located within these samples, which could suggest that some bacteria may have specific relationships with cyanobacteria . However, many of these latter bacteria are also found living independently of cyanobacteria , and the makeup of cyanobacterial-associated communities varies based on the location, type of cyanobacteria, and environmental conditions including nutrient availability and temperature [4–6]. The heterotrophic bacterial community around cyanobacterial blooms appears to be directly influenced by the bloom in that the community structure changes over its progression . In fact, if the cyanobacteria are eliminated by a viral infection, the heterotrophic bacterial community drastically shifts . Conversely, heterotrophic bacteria have also been shown to affect the growth of cyanobacteria. Various strains of bacteria found living with Nodularia spumigena were co-cultured with the cyanobacterium, and several were found to either increase or decrease the growth of the cyanobacterium compared to axenic cultures . Additional studies of heterotrophic bacteria associated with cyanobacterial blooms have verified that co-cultures can increase or decrease cyanobacterial growth . This is likely due to specific interactions of carbon and nutrient exchange . However, the interactions between cyanobacteria and natural assemblages of heterotrophic bacteria involve a large number and variety of interfaces, and are certainly more complex than a specific symbiosis involving two specific partners. Thus, it becomes clear that gaps exist in our knowledge of the microbial communities surrounding cyanobacteria.
Cyanobacteria have been a rich source of bioactive natural products (secondary metabolites and/or toxins), and their biosynthesis has been studied at the chemical, biochemical and genomic levels [11–14]. There is some evidence that the bacterial communities associated with cyanobacteria may affect these biosynthetic processes in different ways. Heterotrophic bacterial communities surrounding cyanobacteria may not only change cyanobacterial growth characteristics, but also have the potential to break down cyanobacterial toxins  or modulate toxin production. For example, toxic Microcystis blooms with different heterotrophic bacteria produce altered microcystins of varying toxicity .
Additionally, in some cases there are uncertainties about which organism is the true producer of a natural product, or if a collaborative biosynthetic effort is required between the cyanobacterium and a heterotrophic bacterium. Considering the complexity of these metabolites and their assembly pathways, it is highly unlikely that the pathways separately evolved in such divergent organisms as cyanobacteria and heterotrophic bacteria. For example, the lyngbyatoxins, a class of potent skin irritants and tumor promoters isolated from field collections of M. producens, show high structural and pharmacological similarity to teleocidin, a metabolite which is produced by Streptomyces species [15, 17]. Similarly, an extract from an assemblage of the cyanobacteria Moorea producens and Tolypothrix sp. yielded the toxin kalkipyrone; this metabolite is closely related to the Streptomyces metabolites actinopyrone and iromycin [18, 19]. Another example is given by swinholide A, an actin-binding toxin originally isolated from the sponge Theonella swinhoei , but subsequently shown to originate from a member of the complex community of heterotrophic bacteria growing within the sponge . However, swinholide A was also isolated from field collections of a marine cyanobacterium along with a glycosylated derivative , initially creating some confusion about the true metabolic source of this complex polyketide. However, recent characterization of closely related gene clusters for swinholide-like molecules from a heterotrophic bacterial symbiont of the sponge, Entotheonella sp., and several cultured cyanobacteria, reveals a complex evolutionary relationship between these pathways, and suggest a mixture of vertical inheritance and convergent evolutionary processes . As these examples illustrate, there is considerable uncertainty concerning the true biosynthetic source of secondary metabolites isolated from cyanobacteria that possess natural assemblages of heterotrophic bacteria. Overall, the study of these cyanobacterial-associated heterotrophic bacterial communities is important as it relates to the ecology and physiology of these organisms as well as the roles and production of their secondary metabolites.
Moorea producens (previously Lyngbya majuscula)  is a filamentous tropical marine cyanobacterium capable of photosynthesis but unable to fix atmospheric nitrogen. Members of this genus are known to be prolific producers of natural products; around 200 secondary metabolites have been isolated from this organism, and the genomes of various strains contain many polyketide synthase and non-ribosomal peptide synthetase genes [23–25]. M. producens has been observed to possess a large community of bacteria on its filaments . However, very little is known about this bacterial community or its inter-relationships and interactions with the cyanobacterial host. One such strain, M. producens JHB, a known producer of the natural products hectochlorin , the jamaicamides , and cryptomaldamide [unpublished], was originally collected from a shallow habitat in Hector’s Bay, Jamaica in 1996. It has been maintained in uni-cyanobacterial culture since this time along with its associated heterotrophic bacterial community. The metagenome of this M. producens JHB strain was sequenced and assembled, followed by extensive binning for cyanobacterial versus heterotrophic bacterial DNA. This process yielded a draft genome of the cyanobacterium along with the essentially complete 5.99 MB genome of a M. producens JHB-associated bacterium. Analysis of this latter bacterial genome, along with experiments to determine its identity and potential function as an associate of M. producens JHB, is the focus of this current report.
Moorea producens JHB (GenBank: FJ151521.1) was collected in Hector’s Bay, Jamaica in August 1996 . M. producens 3 L (NR116539) was collected in December of 1993 at Las Palmas Beach near the CARMABI Research Station in Curaçao, Netherland Antilles, N12 07.387' W68 58.157' . 3 L Oscillatoria (EU244875), identified as Oscillatoria nigroviridis, was isolated as a contaminant of the 3 L M. producens strain. M. bouillonii (FJ041298) was collected in May of 2005 near Pigeon Island in Papua New Guinea, S4 16.063' E152 20.266'. Leptolyngbya sp. (ISBN3Nov94-8, KC207938.1) was collected in November of 1994 near Sulawesi, Indonesia. PAP25Jun12-3 was collected in June of 2012 near Portobello, Panama. All of these were established and maintained as uni-cyanobacterial cultures using standard microbiological isolation techniques [27, 28]. The cultures were grown under static conditions at 28 °C under uniform illumination (4.67 μmol photon s−1 m−2) with a 16 h/8 h light/dark cycle provided by 40 W cool white fluorescent lights. SWBG-11 media contained 35 g/L Instant Ocean (Aquarium Systems Inc.).
DNA extraction and sequencing
DNA was extracted from the harvested biomass of cultures of M. producens JHB, along with its microbiome of heterotrophic bacteria, using the JGI phenol-chloroform protocol . The metagenomic DNA was sequenced using the Illumina HiSeq system, paired end library of 2 × 100 bp. Approximately 12 GB of data were obtained.
Assembly and other bioinformatics
The metagenomic reads were assembled using SPAdes version 3.0.0 . The contigs were binned by GC content, coverage, tetranucleotide fingerprint, and phylogenetic classification of 107 single copy genes. This binning strategy strongly suggested that the six largest non-cyanobacterial contigs most likely belonged to the same taxon. Using Geneious De Novo Assembler (Geneious®), an isolated reassembly of these six contigs resolved the repeated regions and generated a circular scaffold comprised of a single contig that only lacked part of the 16S-ITS-23S rRNA operon. However, previous PCR experiments (as described below) had already provided a single and complete 16S rRNA sequence. The final circular scaffold, including the complete 16S rRNA gene, was submitted for automatic annotation using RAST . Numbers of copies of this complete 16S rRNA gene were confirmed by comparing the coverage of a single copy gene found only in this genome (selA) versus the coverage of the 16S rRNA gene, confirming that a single 16S rRNA gene was present, and most likely, only a single 16S-ITS-23S operon as well. The identified selA gene, which is unique to the Mor1 genome, was used for further experiments as a marker for presence or absence of the Mor1 bacterium. In addition, a more detailed annotation of the Mor1 genome was obtained by submitting the genome to the expert reviewed annotation at JGI (Joint Genome Institute) IMG/ER web platform and to antiSMASH for identification/annotation of secondary metabolite biosynthetic gene clusters .
The assembly of the M. producens JHB genome was performed using a combination of assembly utilizing SPAdes along with a reference assembly to a closed Moorea genome (unpublished). This assembly generated a single scaffold of 9.37 Mb with a 43.5 % GC content. The M. producens JHB genome was submitted to the same annotation tools as Mor1, and comparative genomics and statistics between Mor1, M. producens JHB, and other genomes were developed using Genome Statistics, Search Pathways, COG Homology and the Abundance Profile tools from the JGI (Joint Genome Institute) IMG/ER database.
The relative abundance of M. producens JHB and Mor1 in the overall sequenced metagenomic sample was estimated by the percentage of reads recruited to each of these draft genomes compared to the total number of metagenomic reads (approximately 16 Mb). The genomes were normalized by the average genome size of 3.6 Mb (average size of all 3,777 complete bacterial genomes currently available at JGI database). Similarly, the same percentage was calculated for 421 contigs (maximum size of 10,422 bp, total size of 225,489 bp) not assembled into a genome and not belonging to neither JHB or Mor1 (representing other JHB associates), The recruitment of reads was performed by using Bowtie2 mapping with the option end-to-end and disregarding pair end reads to minimize the exclusion of reads from small contigs. Gene calling using Prodigal was performed and the predicted open reading frames (proteins) were submitted to DarkHorse  in order to infer phylogenetic classification for these open reading frames.
16S rRNA gene location and analysis
Primers designed for use in this study
Tm in °C
5′ -AAGGAGGTGATCCAGCCGCAGG- 3′
5′ -TGAGAGGGTGACCGGCCACACT- 3′
5′ -AGGCGACGATGGGTAGCCGACC- 3′
5′ -CTGGAGAGTTTGATCCTGGCTCAG- 3′
selA Fw 428
5′ -ACTATCGCAAGGCGATCAACAAGA- 3′
selA Rv 1180
5′ -CTAGCTCATCGCTCCTATCAG- 3′
A phylogenetic tree based on this 16S rRNA gene was created, incorporating 16S rRNA sequences from Acidobacteria, Proteobacteria, and Cyanobacteria. 16S rRNA sequences were obtained from GenBank, then aligned using MUSCLE aligner with 5 iterations, gap open score −1 and word size of 5 bp. The tree was built using Geneious Tree Builder, with the Jukes-Cantor genetic distance model, Neighbor-joining tree build method, 100 bootstraps, and Anabaena variabilis ATCC 29413 as the out-group.
Culturing attempts of the associated bacterial community from Moorea producens JHB
Solid media utilized for culturing heterotrophic bacteria associated with M. producens JHB sheaths
0.4 % glucose
Difco Marine Agar
3 % Sigma Sea Salt + 0.4 % mannose + 0.3 % casamino acids
3 % Sigma Sea Salt + 0.4 % mannose + 0.3 % casamino acids
0.5 μM or 2 μM Ferric Ammonium Citrate
1 % starch + 0.2 % yeast extract + 0.4 % peptone
Media mixed with cut up filaments of Moorea producens JHB
Media mixed with freeze dried and ground up filaments of Moorea producens JHB
Bacterial colonies that grew on these plates were isolated and grown overnight in liquid media. DNA was extracted from the overnight cultures using the Wizard Genomic DNA Purification Kit (Promega). PCR was performed on the DNA samples using the selA primers (Table 1), and the 16S rRNA 27 F and 1492R primers . PCR was carried out in 25 μL volumes, containing 12.5 μL of 2x Taq Master Mix, 0.5 μL MgCl2 (25 mM), 1.0 μL of each primer (10 μM), 1.0 μL of DNA template, and 9 μL sterile water. The amplification conditions were as follows: initial denaturation at 95 °C for 4 min, followed by 30 cycles of 95 °C for 30 s, 55 °C for 30 s, and 72 °C for 30 s, followed by a final extension step at 72 °C for 1 min. The 16S rRNA PCR products were then cloned into the pCR 4-TOPO Vector (Invitrogen TOPO TA Cloning Kit) using the standard protocol, followed by sequencing. The obtained sequences were analyzed using BLASTn.
Samples for TEM were prepared using 2 % glutaraldehyde in saltwater (1 h), 2 × 5 min rinses in saltwater, 1 % osmium tetroxide (1 h), 1 × 5 min rinse in 0.15 M cacodylate buffer, 2 × 5 min rinses in ddH20 and 2 % uranyl acetate overnight. This was followed the next day with 2 × 5 min ddH20 rinses. Dehydration was achieved with a graded (20 %, 50 %, 70 %, 90 %, 100 %, 100 %) EtOH series. The samples were then embedded in 50/50 mixture of Spurr’s/EtOH overnight. The next day the samples were incubated in 100 % Spurr’s for 24 h, after which the samples were placed in 100 % fresh Spurr’s for 2 × 1 h and left to polymerize for 48 h. Thin sections (70 nm) were obtained using an Ultracut E microtome (Reichert-Jung, Vienna, Austria) and then placed on 200 mesh fine bar copper grids. The grids were subsequently stained with uranyl acetate and Sato lead. A 1200FX TEM (JEOL, Tokyo, Japan) was used to view the samples.
Semi-quantitative PCR of DNA from washed and unwashed filaments
One sample of JHB filaments was prepared according to the wash protocol specified above in “Culturing trials of the associated bacterial community of Moorea producens JHB”. After centrifugation, the supernatant was removed and the cyanobacterial filaments were used as a “washed filament” sample.
DNA was extracted from the washed filament sample as well as an equivalent mass of unwashed JHB filaments using the Wizard Genomic DNA Purification Kit (Promega) using the standard protocol. PCR was then performed on both samples using the selA primers (Table 1). PCR was carried out in 25 μL volumes, containing 12.5 μL of 2x Taq Master Mix, 0.5 μL MgCl2 (25 mM), 1.0 μL of each primer (10 μM), 1 μL (18.6 ng/μL) of DNA template, and 9 μL sterile water. The amplification conditions were as follows: initial denaturation at 95 °C for 4 min, followed by 28 cycles of 95 °C for 30 s, 55 °C for 30 s, and 72 °C for 30 s, followed by a final extension step at 72° for 1 min. After PCR, the samples were run on a 1 % agarose gel and the intensities of the bands quantified using Gel Quant Express (Life Technologies).
Examination for the presence of Mor1 in other cultures
In order to examine the extent of Mor1 in other laboratory cultures, a possible indication of cross-contamination between cultures, the following were tested for the presence of the selA gene (present in Mor1 but not M. producens; see Results): Moorea producens JHB, Moorea producens 3 L, Moorea bouillonii, 3 L Oscillatoria, Scytonema hoffmani “2846 axenic and xenic,” Leptolyngbya sp. (coded ISBN3Nov94-8), and PAP25Jun12-2. In each case, DNA was extracted from several grams of wet biomass using the QIAGEN Genomic-tip 20/G kit applying the standard protocol. PCR was performed on the extracted DNA samples using the selA primers (sequences indicated in Table 1). PCR was carried out in 25 μL volumes, containing 12.5 μL of 2x Taq Master Mix, 0.5 μL MgCl2 (25 mM), 1.0 μL of each primer (10 μM), 1.0 μL of DNA template, and 9 μL sterile water. The amplification conditions were as follows: initial denaturation at 95 °C for 4 min, followed by 30 cycles of 95 °C for 30 s, 55 °C for 30 s, and 72 °C for 30 s, followed by a final extension step at 72° for 1 min.
Co-culturing of the JHB strain with other cyanobacteria
Matrix of co-culturing experiments involving M. producens JHB and various other filamentous tropical marine cyanobacteria
M. producens JHB
3 L Oscillatoria
M. producens JHB
Single culture control
Mor1 transfer experiment
Mor1 transfer experiment
Mor1 transfer experiment
3 L Oscillatoria
Single culture control
Single culture control
Single culture control
DNA extraction was performed for each sample utilizing JGI’s phenol-chloroform protocol  or the QIAGEN Genomic-tip 20/G kit using the standard protocol. Each DNA sample was then tested for the presence of the 16S rRNA gene (to indicate sample quality) and the selA gene using PCR. Primers 27 F and 781R for 16S rRNA , and selAFw 428 and selARv 1180 were used (Table 1). PCR was carried out in 20 μL volumes, containing 10 μL of 2x Taq Master Mix, 0.5 μL MgCl2 (25 mM), 1.0 μL of each primer (10 μM), 1.0 μL of DNA template, and 6.5 μL sterile water. The amplification conditions were as follows: initial denaturation at 95 °C for 4 min, followed by 30 cycles of 95 °C for 30 s, 50 °C with 16S rRNA or 55 °C with selA for 30 s, and 72 °C for 60 s, followed by a final extension step at 72 °C for 7 min.
The genome of the bacterium Mor1 has been deposited in GenBank under the accession number CP011806.
Results and discussion
Genome assembly and annotation
The non-axenic uni-culture of the cyanobacterium M. producens JHB, originally collected in Hector’s Bay, Jamaica, was sequenced along with its associated heterotrophic bacterial community by Illumina HiSeq sequencing, assembly with SPAdes, binned and reassembled with the Geneious De Novo Assembler. In addition to a single scaffold for the cyanobacterial genome (to be reported separately), this process yielded a 5.99 Mb contig from an associated bacterium. Average coverage of this bacterial contig was 33.6 fold and it possessed a 66.8 % GC content, very different from the 43.5 % GC content of the M. producens JHB genome. Further analysis revealed that the scaffold was circular and lacked only a fraction of the 16S-ITS-23S operon (partial 16S and 23S rRNA genes were present but the full ITS region was absent) comprising 2820 nucleotides between the 5′ and 3′ ends of the circular scaffold. Continued search of the raw sequencing data was unsuccessful to resolve this region. However, sequence data from PCR amplification of the complete 16S rRNA gene was incorporated into the scaffold (hereafter named the Mor1 chromosome).
The assembled complete genome of Mor1 was submitted for rapid automatic annotation through RAST (http://rast.nmpdr.org/), and using RAST’s SEED Viewer, revealed that the genes for photosynthesis or carbon fixation were lacking, thus indicating that it was heterotrophic. Preliminary comparison of the genomes of M. producens JHB and Mor1, again using RAST, revealed several genes present in the bacterium but not in JHB. Of these, the L-seryl-tRNA selenium transferase gene (selA) was selected for use as a specific genetic marker of Mor1, useful for examining the presence of this organism in other cyanobacterial strains. This gene encodes for the tRNA incorporation of selenium-containing cysteine residues in proteins and is not common in cyanobacteria . Additional inspection of the sequenced metagenome revealed that the selA gene was present only in the Mor1 chromosome and as a single copy. Moreover, BLASTN analysis revealed that none of the 30,622 bacterial genomes in the JGI database contains a single sequence with more than 50 % coverage and 90 % identity to the Mor1 selA gene, identifying this gene as an excellent specific genetic marker of this bacterium. Consequently, specific primers were created from the sequence of the selA gene and utilized in later experiments as described below.
Relative abundance and estimated consortium composition
Efforts to culture Mor1 free of M. producens JHB
A number of different kinds of media, as described in the Methods and Table 2, were evaluated for Mor1 cultivation. These culture attempts included numerous nutrient combinations as well as enrichments with iron. In order to provide potentially required growth factors for Mor1 culture that might be found in M. producens JHB, filaments of JHB were cut into short pieces, freeze-dried and ground with a mortar and pestle, and then added to nutrient agar for culturing experiments. Source bacteria for these culture attempts were obtained from the cyanobacterial sheaths by a wash procedure described in the Methods, and bacteria were cultured from the wash buffer. As a result of these trials, dozens of different bacterial cultures were obtained. By 16S rRNA analysis, these included species of the genera Muricauda, Alteromonas, Rhodovulum, and Alcinovorax, as well as Marinobacter salsuginis and a Rhodobacteraceae strain. However, none of the cultured strains were found to possess the selA gene by PCR analysis, and hence, Mor1 was not among the culturable bacteria from M. producens JHB. We propose that Mor1 has nutrient requirements not met by any of these supplemented media types.
Mor1 exists mainly on the exterior of the M. producens JHB sheath
Examination of the specificity of Mor1 on Moorea spp.
Genome comparison between M. producens JHB and Mor1
Strikingly, category K, “Transcription”, is represented by more than double the OGs in the Mor1 genome versus the JHB genome. This is unexpected as it was previously reported that M. producens 3 L (aka L. majuscula 3 L) contains a large number of genes involved in transcription and signal transduction. According to this report, “the numbers and diversity of sigma factors that are global regulators of gene expression in bacteria appear higher in L. majuscula 3 L than in most other cyanobacteria” . Indeed, Moorea producens JHB has the same number of annotated sigma factors as 3 L, 15 in total. Remarkably, the associated Mor1 genome contains 90 sigma-factor genes (the average number of sigma-factor genes among the Acidobacteria genomes currently available at JGI/IMG is 26), 55 of which are annotated as “RNA polymerase sigma-70 factor [a Extra Cytoplasmic Function (ECF) subfamily of factors]. The most important mode of action for ECF sigma in Gram negative bacteria (such as the Acidobacteria) is through Cell Surface Signaling . The other proteins involved in cell surface signaling via the sigma-70 factor are the anti-sigma factor TonB-dependent outer membrane receptor and the TonB-ExbB-ExbD system (see description in reference ). The only other receptors found that can be associated with iron metabolism in Mor1 are annotated as “Outer membrane receptor proteins, mostly Fe transport”. M. producens JHB lacks this ECF Cell Surface Signaling system, thereby suggesting that the iron acquisition and regulation systems are much more sophisticated in Mor1 than M. producens JHB. This hypothesis was explored by adding Ferric Ammonium Citrate to the enriched Sigma Sea Salt media in an attempt to culture Mor1; however, this was unsuccessful.
Lastly, category X [Mobilome (prophages and transposons)] has the most notable difference in gene count between the two bacterial species. The M. producens JHB genome possesses 199 transposases whereas none are found in the Mor1 genome. It has been hypothesized that intracellular bacteria have a tendency to accumulate transposases in early stages of intracellular symbiosis [45, 46]. Therefore, the lack of transposases suggests that Mor1 is not an intracellular symbiont; rather, it appears to be extracellular, which is supported by the previously mentioned decrease in signal of the selA gene signal when semi-quantitative PCR was performed (Fig. 5). Intriguingly, while analyzing the COGs of 26 other Acidobacteria genomes available at IMG/JGI, it was observed that only one other Acidobacterial genome [JGI GOLD ID: Ga0001215] lacks transposases, indicating that this is an uncommon feature within this phylum. Transposases are important for giving genomes the ability to adapt to evolutionary pressures by facilitating horizontal gene transfer or rearranging of the genome . However, obligate pathogens and endosymbionts have lower numbers of transposases . Hence, the absence of transposases in Mor1 suggests that the potential symbiotic relationship with the M. producens JHB strain precludes the need for horizontal gene transfers or rearrangement of the Mor1 genome . Lastly, both M. producens JHB and Mor1 harbor a gene from category X known as ParE. This gene is responsible for plasmid stabilization, thus indicating that both organisms may harbor plasmids, even though contigs encoding for plasmids were only found in association with the M. producens JHB genome (on the basis of similar GC content). However, it was not possible to completely assemble any plasmids from the metagenomic data due to the fragmented nature of the assembly.
With regards to primary metabolism, Mor1 is only prototrophic for the biosynthesis of L-alanine, L-aspartate, L-glutamate, L-glycine, and L-glutamine, as well as for common co-factors such as flavin, coenzyme A, NAD, heme and thiamine. The lack of biosynthetic genes for a number of key primary metabolites, including several essential amino acids, suggests that Mor1 is adapted to thrive in a consortium with other bacteria, such as with M. producens JHB and its microbiome. Specifically, Mor1 lacks biosynthetic genes for several important amino acids: the aromatic amino acids Phe, Tyr and Trp, the positively charged amino acids Lys, Arg and His, and all non-polar amino acids except glycine and alanine. Complementing this, however, is the occurrence in the Mor1 genome of several transporters that are annotated as “amino acid/polyamine/organocation transporter (APC superfamily)”, “amino acid/amide ABC transporter substrate-binding protein (HAAT family)”, and “amino acid transporter”.
Furthermore, it is not capable of cobalamin or biotin biosynthesis, a metabolic insufficiency clearly revealing its dependency on other organisms for survival. Interestingly, a transporter for the uptake of cobalamin was identified in both Mor1 and M. producens JHB, which also lacks the capacity for biotin synthesis; this indicates that other bacteria in the consortium are likely providing this key co-factor. Because Mor1 possesses the genes for the biotin carboxyl carrier protein and biotin ligase, biotin is clearly required, but is presumably acquired through uptake from the environment.
The sequencing effort of the M. producens JHB metagenome revealed a 5.99 Mb genome of an unknown, uncultured heterotrophic bacterium, named here as Mor1. The organism belongs to the phylum Acidobacteria, subgroup 22, but is unable to be taxonomically further classified, and as of yet, has not been successfully cultured. A comparative genomics study generated several hypotheses regarding the potential relationship between the M. producens JHB and Mor1. Four main areas of interest emerged from this analysis: transcriptional regulation, iron metabolism, nitrogen cycling between the two microbial species, and a complete lack of transposases in the Mor1 genome. Examination for the presence of Mor1 in various laboratory cultures, along with co-culturing experiments to evaluate the transferability of Mor1 to other cyanobacteria, support the idea that it is a specific associate of some strains of M. producens.
Because all natural products investigations of M. producens JHB to date have occurred using cultured non-axenic biomass which is comprised of cyanobacterial filaments and its associated microbiome, there remains the possibility that some of the identified secondary metabolites (e.g. jamaicamide, hectochlorin) are actually produced by Mor1 or another associated bacterium. Because we have not been able to cultivate Mor1 or the cyanobacterium independent of one another, we are not able to answer this question using chemical methodologies. However, several lines of evidence support the conclusion that these natural products are of cyanobacterial origin: 1) their chemical structures are consistent with pathways known for cyanobacterial natural products, 2) they are produced in relatively high yield per unit of biomass, 3) their biosynthetic pathways use motifs, codons, and GC content consistent with cyanobacterial pathways, and 4) new to this reported work, the major associated heterotrophic bacterium, Mor1, lacks the genes for these metabolic pathways. In fact, only two secondary metabolite pathways were detected in Mor1 based on an antiSMASH analysis of its assembled genome , and neither of these is predicted to produce a compound thought to be of cyanobacterial origin.
To further characterize the potential symbiotic relationship between Mor1 and M. producens, additional effort is needed to culture M. producens and Mor1 independently of one another. Growth rates of M. producens with and without Mor1 might infer a symbiotic interaction of these two microbial species [8, 9]. Interaction between these two organisms involving nutrient exchange or signaling molecules could be examined via a transcriptomic analysis , imaging mass spectrometry , or further chemical analyses. Overall, this work reveals that niche environments such as the sheaths of tropical marine cyanobacteria may be rich locations in which to prospect for novel microbial species with potentially useful biotechnology applications.
The work was supported by the NIH grants CA108874 and GM107550. A.K. was supported in part by the Russian Science Foundation (grant 14-50-00069). T.F.L. was funded by a CAPES Foundation Fellowship, n° 13425137, Ministry of Education of Brazil.
Availability of data and materials
The genome of the uncultured bacterium Mor1 was deposited in Genbank. Accession number CP011806.
SLC designed experiments, performed all the co-culture experiments, made figures and wrote the manuscript; DB designed experiments, determined distribution of Mor1, performed isolation experiments using different conditions, made figures and co-wrote manuscript; TFL performed genomic comparison bioinformatics, made figures and co-wrote manuscript; AK assembled the genome and edited manuscript; NE provided electron micrographs (EM) figures and edited manuscript; EG provided cultures and edited manuscript; WHG designed experiments and edited manuscript; LG designed experiments, provided guidance to SLC, DB and TFL and co-wrote manuscript. All authors read and approved the final manuscript.
The authors declare that they have no competing interests.
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