- Open Access
Physiologic and metabolic characterization of a new marine isolate (BM39) of Pantoea sp. producing high levels of exopolysaccharide
© Silvi et al.; licensee BioMed Central Ltd. 2013
Received: 19 December 2012
Accepted: 27 January 2013
Published: 29 January 2013
Marine environments are the widest fonts of biodiversity representing a resource of both unexploited or unknown microorganisms and new substances having potential applications. Among microbial products, exopolysaccharides (EPS) have many physiological functions and practical applications. Since EPS production by many bacteria is too scarce for practical use and only few species are known for their high levels of production, the search of new high EPS producers is of paramount importance. Many marine bacteria, that produce EPS to cope with strong environmental stress, could be potentially exploited at the industrial level.
A novel bacterium, strain BM39, previously isolated from sediments collected in the Tyrrhenian Sea, was selected for its production of very high levels of EPS. BM39 was affiliated to Pantoea sp. (Enterobacteriaceae) by 16S rRNA gene sequencing and biochemical tests. According to the phylogenetic tree, this strain, being quite far from the closest known Pantoea species (96% identity with P. agglomerans and P. ananatis) could belong to a new species. EPS production was fast (maximum of ca. 21 g/L in 24 h on glucose medium) and mainly obtained during the exponential growth. Preliminary characterization, carried out by thin layer and gel filtration chromatography, showed that the EPS, being a glucose homopolymer with MW of ca. 830 kDa, appeared to be different from those of other bacteria of same genus. The bacterium showed a typical slightly halophilic behavior growing optimally at NaCl 40 ‰ (growing range 0-100 ‰). Flow cytometry studies indicated that good cell survival was maintained for 24 h at 120 ‰. Survival decreased dramatically with the increase of salinity being only 1 h at 280 ‰. The biochemical characterization, carried out with the Biolog system, showed that MB39 had a rather limited metabolic capacity. Its ability, rather lower than that of P. agglomerans, was almost only confined to the metabolization of simple sugars and their derivatives. Few alcohols, organic acids and nitrogen compounds were partially used too.
Strain BM39, probably belonging to a new species, due to its remarkable EPS production, comparable to those of known industrial bacterial producers, could be suggested as a new microorganism for industrial applications.
Oceans and seas are the widest sources of biological and chemical diversity representing a prolific reserve of unexploited and/or unknown microorganisms [1, 2]. Thus, marine environments are great resources of new substances having potential applications in pharmaceutical, feed and food, fine chemicals and enzyme industries [2, 3]. The search of new microorganisms, having unique physiological and metabolic capabilities, aids to better comprehend the ecosystem and provides opportunities to discover new compounds of commercial importance. This is particularly true for marine bacteria that have been less studied than their terrestrial counterpart and are often underrated or completely ignored by many scientists [4, 5].
Among the microbial products, exopolysaccharides (EPS) have many important physiological functions and various practical applications deductible from their roles in nature.
These high molecular weight polymers represent essential components of the secreted extracellular material and are involved in various cell function such as: cell protection from freezing, dehydration and antimicrobial agents [6–9]; adhesion to surfaces, other organisms and biofilm production ; support in pathogeny and virulence [11, 12]; inhibition of biofilm formation [13, 14]; storage of reserve carbon sources .
EPS find applications in environmental biotechnology being employed in soil and water bioremediation, decontamination and detoxification [15–18]. Moreover, they are used in pharmaceutical/biomedical [19, 20], cosmetic , chemical [22, 23] and food industries [24, 25].
The amount of EPS produced by many bacteria, few grams per liter, is too low for their practical use. By contrast, only few species are known for their high levels of production. Among them, strains of Xanthomonas campestris, Bacillus polymyxa, Klebsiella pneumonie and Sfingomonas elodea are the most studied and only few are used at the industrial level [16, 26–29].
Different microorganisms produce EPS with diverse composition and having different characteristics leading to their employment in diversified ambits [12, 16]. In addition, same microorganism could release EPS with different composition when grown in different conditions . In this context, the search of new high EPS producers is still important to find new applications or better fit traditional uses. Moreover, strain physiologic and metabolic characterization is extremely useful to understand and optimize microbial productions [30, 31].
In marine environment many bacteria, producing EPS to cope with strong environmental stress and to survive adverse conditions [32–34], represent promising sources of species to be exploited at the industrial level.
In this study, we report on the detailed metabolic characterization of a new slight halophilic marine bacterium producing high levels of exopolysaccharide. The strain was identified as Pantoea sp. by 16S rRNA gene sequencing and biochemical tests. Time course of EPS production and partial chemical characterization of the polymer are also reported. In addition, physiologic adaptation to salinity is also studied by both cultural methods and flow cytometry.
Results and discussion
The isolate, subjected to 16S rDNA sequence analysis (1266 bp), was affiliated to the genus Pantoea. Its sequence, GeneBank accession number “BankIt1581807 Pantoea KC163803”, matched with entries with similarities ranging from 96 to 98%. However, matching with known species of Pantoea was 96% only; thus, due to the low similarity, BM39 assignment to the species level was not possible.
The uncertain affiliation of BM39 was observed by the Biolog system too. The information obtained did not consent the attribution to species included in the database being P. agglomerans, the closest species with 51% of similarity only.
Growth and physiological state at different salinities
Traditionally, strict definition of “marine microorganism” implies that a marine species must be found only in marine environments [40, 41]. Even if many species are just confined in marine environments, others, widely diffused in terrestrial environments, present strains that are well adapted to marine conditions . Thus, it is difficult to understand if a microorganism, isolated from sea samples could be defined as “marine”. Actually, the isolate could be a strict marine microorganism, an adapted strain from other environments or a microorganism accidentally found still alive in the sea but non-adapted to marine conditions.
The microorganism, thus defined as slight halophilic, appears well adapted to a rather broad range of salinity but growth far from optimal conditions required more time probably for more complex homeostasis regulation.
More detailed information concerning homeostasis and physiological state of each bacterial cell, submitted to different conditions of salinity, had been obtained by flow cytometry in the range 0-280 ‰.
In this context, remarkable differences were recorded, during the experiment progression, in relation to salinity. As expected, optimal conditions were confirmed at 40 ‰. In fact, this is the sole situation showing all cells in complete viable state (strong DiOC6, only) after 24 h of incubation. Cells started to die, for possible initial starvation, around the 48 h to be in advanced dead phase at 72 h (Figure 3b).
Similar behavior was recorded both at 0 and 80 ‰ even if signs of cell sufferance were more evident at 48 h, in particular at 80 ‰ (Figure 3a, c). The progressive increase of salinity proportionally determined the increase of cell sufferance. This is particularly evident at 280 ‰; in this case, after only 2 h, almost all cells were died or dying (Figure 3f).
Metabolism of different carbon sources
Comparison between the metabolic competences of Pantoea sp. BM39 and other Pantoea species as revealed by the Biolog system
α-Cyclodextrin, dextrin, glycogen, N-Acetyl-D-galactosamine, adonitol, i-erythritol, L-fucose, lactulose, D-raffinose, D-sorbitol, xylitol
N-acetyl-D-glucosamine, L-arabinose, D-fructose, D-galactose, α-D-glucose, maltose, D-mannitol, D-mannose, sucrose, D-trehalose,
D-arabitol, D-psicose, turanose
α-D-lactose, D-melibiose, β-A-26-methyl-D-glucoside
Succinic ac. methyl-ester, acetic ac., formic ac., D-galactonic ac. Lactone, D-glucosaminic ac., α-OH-butyric ac., β-OH-butyric ac., γ-OH-butyric ac., p-OH-phenylacetic ac., itaconic ac., α-keto butyric ac., α-keto glutaric ac., α-keto valeric ac., propionic ac., quinic ac., D-saccharic ac., sebacic ac., bromosuccinic ac., succinamic ac., glucuronamide
Pyruvic ac. methyl ester, D-gluconic ac., D, L-lactic ac.
Cis-aconitic ac., D-glucuronic ac., D-galacturonic ac.
Citric ac., succinic ac.
L-alaninamide, L-alanylglycine, L-asparagine, glycyl-L-aspartic ac., glycyl-L-glutamic ac., L-histidine, OH-L-proline, L-leucine, L-ornithine, L-phenylalanine, L-pyroglutamic ac., L-threonine, D,L-carnitine, γ-amino butyric ac., urocanic ac.,
D-alanine, L-alanine, L-aspartic ac., L-proline, D-serine
Phenyethylamine, putrescine, 2-aminoethanol, 2,3-butanediol
Inosine, uridine, thymidine
Production of EPS and partial polymer characterization
Kinetic parameters of EPS production by Pantoea sp. BM39 cultivated in shaken cultures on different media
Since medium has not been optimized yet and process had been carried out in shaken flasks, the EPS production by BM39 could be considered already very high. It is worth noting that, as reported for many other processes, microbial productions could be strongly improved by accurate medium formulation and culture condition optimization [31, 46–49]. Our strain production could be considered quite good also in relation to other already studied bacteria. Various known producers release just few g/L of EPS and rarely exceed the amount of 10 g/L [26, 27, 29, 50–52]. Few others, produce much higher levels of EPS comparable with those of BM39 or even higher. However, the high production was often obtained after optimization to increase strain performance [28, 53]. For example, P. agglomerans (Enterobacter agglomerans) strain CRDA 312 produced 27.5 g/L of EPS  but the production was achieved in stirred bioreactors that generally consent better performances in relation to same process carried out in shaken flasks .
Preliminary EPS characterization, carried out by thin layer chromatography after acid hydrolysis, showed that the polymer was constituted only by monomeric units of glucose (data not shown). This justifies the better performance of EMG in comparison with the other media tested. Very likely, glucose is directly used to assemble the biopolymer while fructose and sucrose need a bioconversion before EPS formation. Apparent molecular weight of the polymer, determined by gel permeation chromatography, was 830 kDa.
It is worth noting, that other known species of Pantoea produce EPS with different composition and characteristics. For example, P. stewartii is note to produce “stewartan” a heteropolymer of glucose and galactose . P. agglomerans KFS-9 produces a heteropolymer constituted by arabinose, glucose galactose and gulcuronic acid with a molecular weight of 760 kDa . However, BM39 production was obtained on media containing glucose, fructose or sucrose. It is possible that, on other carbon sources, EPS with different composition and characteristics could be obtained.
Pantoea sp. strain BM39, probably belonging to a new slightly halophilic marine species, showed rather broad euryhaline behavior growing up to ca. 100 ‰ of salinity. The bacterium was able to rapidly produce quite high levels of a homopolymeric glucose EPS that, being different from those of other bacteria, could have different applications. EPS production is comparable with those of known industrial strains and, taking into account that the process has not been optimized yet, BM39 could be considered very promising for the exploitation at the industrial level.
Plate Count Agar (PCA), Yeast extract (YE); Bacto-Tryptone (BT), Mycological Peptone, Luria Bertani broth (LB) and LB agar (LBA) were from Difco (USA). All other chemicals were of analytical grade.
Microorganism and culture conditions
Pantoea sp. BM39 was previously isolated from sediments sampled at 20 m deep in the Tyrrhenian Sea off the coast of Civitavecchia, Roma, Italy . During the study the strain was maintained on PCA at 4°C and subcultured when necessary.
Inocula were prepared suspending some loopful of the bacterium from a PCA plate in 250 ml Erlenmeyer flasks containing 50 ml of LB. Flasks were shaken cultured overnight at 180 rpm and 28°C.
Media for EPS production were as follows (g/L): NaNO3, 5.0; KCl, 0.5; KH2PO4, 1.0; FeSO4 x 7H2O, 0.01; CaCO3, 35.0; Mycological Peptone, 1.0 added with glucose 80.0 (EMG) or sucrose 80.0 (EMS) or fructose 80.0 (EMF).
For EPS production, 250 ml Erlenmeyer flasks, filled with 50 ml of each medium, were added with the bacterial inoculum produced as above (0.150 OD600) and shaken cultured (180 rpm, 28°C) for 72 h. Samples were collected every 6 h. Experiments were done in triplicate.
Media for determination of optimal salinity for growth were prepared adding the necessary amounts of NaCl (from 0 ‰ to 120 ‰, step 10 ‰) to BT 1% and YE 0.5% (LB without NaCl).
For determination of optimal salinity for growth, 250 ml Erlenmeyer flasks, filled with 50 ml of each medium, were added with the bacterial inoculum produced as above (0.300 OD600) and shaken cultured (180 rpm, 28°C) for 36 h. Samples were collected every 1 h during the first 15 h and every 3 h thereafter. Experiments were done in triplicate.
All media were autoclaved at 121°C for 20 min.
Morphological, physiological and biochemical characterization
Tests were carried out on early exponential phase cells from cultures grown at 28°C. Morphological characterization was done using Gram stained cells. Gram staining was carried out using a commercial kit (Merck, Germany) following manufacturer’s instructions. Strain dimensions were obtained using a Leitz Laborlux 11 microscope bearing a micrometric ocular calibrated with a micrometric slide (Leitz Wetzlar, Germany). Catalase and oxidase tests were performed as previously described [56, 57]. Briefly: for oxidase activity, Kovacs reactive (1% of N,N,N,N tetrametil-p-phenylenediamine in water) was added to a fresh colony. After 60 seconds, develop of violet color means positive reaction. For catalase, H2O2 (3%) was added to a fresh colony: bubbles of O2 production meant a positive reaction.
Extended metabolic competences were investigated testing the strain ability to use 95 different compounds (including carbohydrates, carboxylic acids, polymers/oligomers, amines/amides, aminoacids and other compounds) as sole carbon source by the “Biolog” system [30, 58, 59] according to the manufacturer’s directions; results were interpreted with the most recent Biolog Microlog database (Biolog, Hayward, CA, USA).
Strain identification and phylogeny
The strain was identified by analysis of the sequences of the gene encoding for the 16S rRNA. Bacterial genomic DNA was extracted and used for amplification by polymerase chain reaction. Products of amplification were sequenced and compared with databases sequences. Taxonomical information was also obtained by the above mentioned Biolog data base.
DNA extraction and polymerase chain reaction for amplification of the 16S rRNA gene
BM39 grown for 24 h on PCA plates, was used for genomic DNA extraction by thermal shock as follows : a single colony suspension (in 14 μl of sterile deionized water) was heated at 100°C for 5 min, immediately cooled in ice and centrifuged at 4000 g for 3 min. The supernatant was used for PCR reaction. Amplifications were performed in a reaction mixture (final volume 25 μl) containing 2x BioMix (BioLine GmbH, Germany), 15–20 ng/μl of DNA template and 5 pmol/μl of the following universal primers 1389r (ACGGGCGGTGTGTACAAG) and 63f (CAGGCCTAACACATGCAAGTC) (Sigma-Aldrich, USA). Amplification was carried out using a MiniCycler™ (MJ Research, USA) equipped with a heated lid as follows: denaturation at 95°C for 5 min; denaturation at 95°C for 45 s; annealing at 55°C for 1 min; extension at 72°C for 90 s; final extension at 72°C for 7 min; cold-storage 4°C. Step 2, 3 and 4 were repeated for 30 cycles.
PCR products were visualized by electrophoresis on agarose gel (1.0%) prepared with 0.50 g of agarose (Starlab GmbH, Denmark) dissolved in 50 ml of TAE buffer 1X (40 mM Tris-acetate, 1 mM EDTA, pH 8.3, Brinkmann Instruments, Inc., USA) added with 5 μl of GelRed (10,000x, Biotium, USA). Loading was carried out by adding 1 μl of Loading Dye (6x, New England Biolabs, USA) to 5 μl of each sample. The DNA Ladder GeneRuler™ 100 bp (FERMENTAS, Lithuania) was used to quantify PCR products dimension by comparison. The products were purified using Nucleospin Extract kit (Macherey-Nagel, Germany). Sequencing reactions were performed by Macrogen sequencing service (Macrogen Inc., Korea). Sequence assembly was done using the software Chromas (version 1.5 2009, Technelysium Pty Ltd, Australia). Sequences with high similarity available in NCBI GenBank were identified using BLASTn search.
BM39 sequence was deposited to NCBI/GenBank database with the “BankIt1581807 Pantoea KC163803” accession number.
Alignment and tree reconstruction
Automatic alignment was first carried out using CLUSTALX , then exported to MEGA4  and improved manually. Phylogenetic tree was reconstructed by neighbor-joining algorithm and maximum composite likelihood model. The robustness of the phylogenetic inference was estimated using the bootstrap method  with 1000 pseudo-replicates.
Exopolysaccharide determination and partial characterization
Bacterial cells and CaCO3 were removed by centrifugation (15 min at 6000 rpm). After removing possible residual CaCO3 from culture supernatant with 1 N HCl, EPS concentration was determined by precipitation at 4°C adding 2 volumes of absolute ethanol. Precipitated EPS was filtered on pre-weighed Whatman GF/D discs, filters were then dried at 95°C for 24 h, cooled into a desiccator and weighed.
For characterization, EPS was recovered by precipitation as above. Precipitate was collected and re-dissolved in distilled water: the procedure (precipitation, centrifugation and re-dissolution in water) was repeated twice. The final aqueous solution was dialyzed against distilled water (24 h at 4°C) freeze-dried, and weighed .
EPS was hydrolyzed with 2 N sulfuric acid at 100°C for 3 h. Then, the solution was neutralized with 1 N NaOH and filtered (Whatman discs, 0.45 μm). Sugar components were identified by thin-layer chromatography (TLC): sugar standards were used for identification.
Thin-layer chromatography (TLC) was performed on silica gel plates 60 F254 (Merck, Darmstadt, Germany) saturated with 0.5 M KH2PO4 using a solvent system of lactic acid (7.4 g/L of distilled water), 2-propanol and acetone in a ratio of 5:1:10. Sugar spots were visualized by spraying the plates with a solution made up of 96 ml of 0.2% naphthoresorcinol solution in ethanol plus 4 ml of concentrated sulfuric acid and incubation at 100°C for 5 min.
EPS apparent molecular weight was determined by gel permeation chromatography as described previously with slight modifications . Briefly, a chromatographic Superose-6 column connected to a FPLC system (Pharmacia) was used for determination after calibration with commercial dextrans (48.6, 80.9, 147.6, 273.0, 409.8, 667.8 and 1400.0 kDa by Sigma-Aldrich).
Flow cytometry analysis
The study has been carried out by the “Servicio de Biologia Fundamental, Centro de Instrumentacion Cientifica”, University of Granada, Granada, Spain using a FACSCanto II cytometer (Becton Dickinson, San José, CA, USA). The cytofluorimeter (CF) was equipped with three laser sets (405, 488, and 625 nm) and detectors for forward-scatter, side-scatter and eight fluorescence colours. Acquisition from the CF and data analysis was done by the FACSDiva v6.1.3 software (Becton Dickinson).
Cells grown for 24 h at 28°C on LBA plates, containing 40 ‰ of NaCl, were harvested and suspended (108 cell/ml) in 40 ‰ NaCl in distilled water. From this concentrated suspension the necessary amount of cells were taken and re-suspended in LB, containing different amount of NaCl (range 0-280 ‰, step 40 ‰), to reach a final bacterial concentration of 106 cell/ml. The various suspensions were incubated in an orbital shaker (28°C and 180 rpm) for 72 h. Samples, taken after 0, 1, 2, 4, 8, 12, 24, 48 and 72 h, were added with propidium iodide (PI) and 3,3-dihexylocarbocyanine iodide (DiOC6) or fluorescein diacetate (FDA) to reach final concentration of 1.0, 0.005, 2.0 μg/ml, respectively. After 15 min of incubation at 28°C stained samples were submitted to the multi-parameter FC and analysed.
The physiological state of the bacterium individual cells was characterized adding different combinations of the fluorogenic dyes as follows. Presence of both an intact polarized cytoplasmic membrane and active transport systems, essential for a fully functional cell, was tested by the addition of PI and DiOC6. PI binds to DNA, but cannot cross an intact cytoplasmic membrane, and DiOC6 accumulates intracellularly when membranes are polarized or hyperpolarized [30, 65, 66]. In addition, cell viability has been tested using the combination of PI and FDA . FDA is actively transported into the viable cells and is converted by membrane esterases into a fluorogenic compound (emission at 530 nm): cell having good homeostasis (viability) are fluorescent. As said PI enters damaged membranes and indicate dying or dead cells.
Statistical analysis of data
One-way analysis of variance (ANOVA) and pair-wise multiple comparisons procedure (Tukey test) were carried out using the software SigmaStat (Jandel Scientific, CA, USA).
The authors wish to thank Dr. Jaime Lazuen of the “Servicio de Biologia Fundamental, Centro de Instrumentacion Cientifica”, University of Granada, Granada, Spain, for the kind support in flow cytometry analysis.
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