Next Article in Journal
Tipping Points in Seaweed Genetic Engineering: Scaling Up Opportunities in the Next Decade
Previous Article in Journal
Conotoxins Targeting Nicotinic Acetylcholine Receptors: An Overview
Article Menu

Export Article

Mar. Drugs 2014, 12(5), 3005-3024; doi:10.3390/md12053005

Fermentation Technologies for the Optimization of Marine Microbial Exopolysaccharide Production
Ilaria Finore 1, Paola Di Donato 1,2, Vincenza Mastascusa 1,2, Barbara Nicolaus 1 and Annarita Poli 1,*
Consiglio Nazionale delle Ricerche (C.N.R.), Institute of Biomolecular Chemistry, Via Campi Flegrei 34, 80078 Pozzuoli, NA, Italy
Department of Sciences and Technology, University of Naples, “Parthenope” Centro Direzionale Napoli (Isola C4), 80143 Naples, Italy
Author to whom correspondence should be addressed; Tel.: +39-081-867-5311; Fax: +39-081-804-1770.
Received: 3 February 2014; in revised form: 2 April 2014 / Accepted: 3 April 2014 / Published: 22 May 2014


: In the last decades, research has focused on the capabilities of microbes to secrete exopolysaccharides (EPS), because these polymers differ from the commercial ones derived essentially from plants or algae in their numerous valuable qualities. These biopolymers have emerged as new polymeric materials with novel and unique physical characteristics that have found extensive applications. In marine microorganisms the produced EPS provide an instrument to survive in adverse conditions: They are found to envelope the cells by allowing the entrapment of nutrients or the adhesion to solid substrates. Even if the processes of synthesis and release of exopolysaccharides request high-energy investments for the bacterium, these biopolymers permit resistance under extreme environmental conditions. Marine bacteria like Bacillus, Halomonas, Planococcus, Enterobacter, Alteromonas, Pseudoalteromonas, Vibrio, Rhodococcus, Zoogloea but also Archaea as Haloferax and Thermococcus are here described as EPS producers underlining biopolymer hyperproduction, related fermentation strategies including the effects of the chemical composition of the media, the physical parameters of the growth conditions and the genetic and predicted experimental design tools.
exopolysaccharides; extremophiles; fermentation; marine microorganisms; statistical tool

1. Introduction

The aquatic habitats represented by the oceans, seas and lakes are the widest sources of biological and chemical diversity that not only constitute a productive reserve of unexploited and/or unknown microorganisms [1,2,3] but are also a great resource of new biomolecules displaying potential biotechnological applications in pharmaceutical, medical [4], cosmetic [5], feed, food and enzyme industries [6]. The singleness of these new microorganisms makes them ideal candidates as models to study the ecosystem apart from providing opportunities to discover new compounds of commercial importance. Among the microbial products, exopolysaccharides (EPS) possess significant main physiological functions and various practical applications. During the last years, the increased demand for new and natural polymeric materials by several industrial fields, such as pharmaceutical, food and others, has moved the interest to the polysaccharides produced by microorganisms. Moreover, EPSs find applications in environmental biotechnology where they are employed in soil and water bioremediation, decontamination and detoxification processes [7,8]. These polymers differ from others that are derived from plants or algae, for numerous valuable qualities. Although the world market is dominated by polysaccharides derived from plants and marine macroalgae, there are many microorganisms (Gram-positive and Gram-negative Bacteria, Archaea, Fungi and some microscopic Algae) that are able to produce polysaccharides as extracellular polymers [9]. Bacterial EPSs that are widely used in food, pharmaceutical and chemical industries as bioflocculants, bioabsorbents, drug delivery agents, etc. are produced by Xanthomonas, Leuconostoc, Pseudomonas, Alcaligenes genera, which synthesize xanthan, dextran, gellan, curdlan. Despite the wide diversity of microbial EPS scenario, xanthan and gellan are the only two EPSs of microbial origin that are used as additives in the food industry in the United States and Europe [10].

Although diverse microbial exopolysaccharides (EPS) have been studied during the last years, little information is available regarding their hyperproduction. In this review, we describe some microbial EPS producers and the related fermentation strategies and genetic tools adopted in order to enhance the EPS yields. We also go through the features of the EPS production process which can vary in order to increase the yield of polymer. Several factors can affect this complex process: For instance, the medium composition and the fermentation conditions (temperature, pH, aeration, etc.) represent variables that act to improve the polymer release. Moreover, since this process is genetically determined, several studies and strategies are being developed to intervene at the genome level with the aim to boost EPS productivity.

2. General Information of Microbial Exopolysaccharides: Chemical Structure, Ecological Role and Biosynthesis

EPSs are divided into two main groups, homopolysaccharides and heteropolysaccharides. The first are made up of a single type of monosaccharide: This is the case, for example, for levan or dextran. Heteropolysaccharides containing three or four different monosaccharides display a backbone structure made up of a repeating unit constituted by ten or less monomers [11]. The most common units constituting the EPSs from marine microorganisms are d-arabinose, d-ribose and d-xylose as pentoses; d-glucose, d-galactose, d-mannose, d-allose, l-rhamnose and l-fucose are found as hexoses, while d-glucosamine, d-galactosamine, d-glucuronic acids and d-galacturonic acids are found as amino sugars and uronic acids, respectively. Other organic or inorganic substituents, such as phosphate, sulfate, succinic, acetic and pyruvic acids can also be found [12]. Several are the examples of polymers with a linear structure and a molecular weight between 1 × 105 to 3 × 105 Da [13]. Some EPSs are neutral polymers but many of them are polyanionic because of the presence of ketal-linked pyruvate or inorganic residues such as phosphate or sulfate or uronic acids. Moreover, the 1,4-β- or 1,3-β- linkages between monosaccharides are most commonly found in the rigid backbone of EPSs while the 1,2-α- or 1,6-α- linkages are typical for the more flexible ones [14].

EPSs are produced in response to biotic stress (e.g., competition), abiotic stress factors (e.g., temperature, light intensity, pH, salinity) and/or as a strategy of adaptation to an extreme environment like in the case of acidophilic or thermophilic species belonging to the Bacteria and Archaea domains [10]. The physiological role of EPS depends on the natural environment in which the microorganisms live. Most of the functions ascribed to EPSs are of protective nature. They could support the microorganisms to tolerate extreme conditions such as extremely high or low temperatures, salinity and limited availability of nutrients by surrounding the cells and their immediate environment [11]. In addition, they are involved in various cell functions such as adhesion to surfaces and to other organisms, in biofilm production, as a support in pathogenic and virulence mechanisms or as storage of reserve carbon sources.

EPS biosynthesis includes three main phases: assimilation of a carbon substrate, intracellular synthesis of the polysaccharide and its exudation out of the cell [15]. Although the exopolysaccharide production is a process that involves a noticeable energy cost, due to the strong need of carbon input for the microorganisms, the gain coupled with their presence is considerably higher compared to the costs (considering the growth increase and the survival of the microbial producers) [16,17]. The mechanism of EPS biosynthesis depends on the type of polysaccharide. In the case of homopolysaccharides (dextran, levan and mutan, etc.), the polymerization reaction occurs thanks to an extracellular glycosyltransferase that is able to transfer a monosaccharide unit from a disaccharide by increasing the length of the polysaccharide chain. In the case of heteropolysaccharides with repeating units, the assembly of repeating units takes place in the cytoplasm through the action of specific glycosyltransferases responsible for the continuous transfer of sugar residues to a lipophilic carrier. Once formed, the sugar chain is transferred outside the cells and polymerized. The extent of the release of the polymers and their eventual chemical modification, i.e., acetylation or pyruvylation reactions, and the addition of phosphate or sulfate substituents are under enzymatic and genetic control. For instance, the knowledge of the glycosyltransferase gene map has been useful in predicting the structure of the repeating unit of EPS in lactic acid bacteria [18,19,20]. Since the microbial EPS production is related to a specific gene cluster, the knowledge of the genome sequence of EPS producers is surely the crucial point for the optimization of their biosynthesis through a system biology approach [21,22]. In addition, the manipulation of genes responsible for the EPS biosynthesis could interfere with the chemical-physical characteristics of EPSs and finally with the properties and potential application of these polymers. However, the regulation of EPS biosynthesis, overall in marine EPS producers, is still very poorly understood: More knowledge on the genetics and biochemistry of EPS biosynthesis is needed in order to engineer polysaccharide properties by modifying production, composition and chain length [23].

3. Marine EPS Producers: Conventional and Non-Conventional (Extremophile) Microorganisms

The marine habitats represent a vast source of natural products, and their microbial inhabitants have developed unique metabolic and physiological capabilities to produce novel metabolites [6,24]. Although more than 10,000 metabolites with biological activities have been isolated from marine microorganisms, most of the marine microbial world remains unexplored [6].

Kumar et al. [9] isolated the species Planococcus maitriensis Anita I from the coastal sea water area of Bhavnagar (India). This microorganism was able to produce an EPS possessing an oil spreading potential comparable to Triton X100 and Tween 80, thus resulting in being suitable for bioremediation, enhanced oil recovery and cosmetic applications.

Iyer et al. [25] described an acidic EPS with a high content of uronic acid, named 71a, produced by Enterobacter cloacae collected from marine sediments in India. The EPS 71a showed emulsifying properties comparable to commercial gums. Mancuso et al. [2,26] described the effect of growth temperatures on the EPS production by the strains CAM025 and CAM036, two marine bacteria isolated from sea ice and seawater sampled in the Southern Ocean (Antarctica) and belonging to the genus Pseudoalteromonas.

A branched EPS that has gelling properties was produced by the Pseudoalteromonas strain HYD 721 isolated from a deep-sea hydrothermal vent of the East Pacific Rise [27], while an EPS with a high degree of acetylation that showed flocculation behavior and a bio-sorption capacity was produced by the Pseudoalteromonas strain SM9913 isolated from deep-sea sediments in the gulf of the Yellow Sea (China) [28,29]. The structure of a highly complex alpha-mannan polymer and its ecological role as crioprotector of a novel EPS from the arctic sea ice bacterium Pseudoalteromonas sp. strain SM20310 was described by Liu et al. [30].

Other cases of microorganisms with an appreciable capability to produce EPS include Gamma-Proteobacteria, species belonging to Idiomarina and Alteromonas genera, in particular Alteromonas hispanica and also species belonging to the Alpha-Proteobacteria group, like Salipiger mucosus and Palleronia marisminoris [31]. Vincent et al. [32] described the isolation of Alteromonas sp. from the epidermis of a polychaete annelid, Alvinella pompejana, living in the deep sea hydrothermal vents of the East Pacific Rise, able to produce a heteropolysaccharide with high levels of uronic acids and pyruvate, and showing anticoagulant and bone healing properties [33,34,35]. Bozzi et al. [36,37] described an EPS capable of binding heavy metals produced by the Alteromonas strain 1644 isolated from Alvinellidae collected from the East Pacific Rise. The marine bacterium Pseudomonas sp. strain S9 was found to produce EPS during both growth and total energy source and nutrient starvation [38]. Lim et al. [39] described the physicochemical properties of some EPSs (capsular and water soluble polysaccharides) produced by the marine bacterium Zoogloea sp. KCCM10036: These EPSs showed an excellent flocculating activity. Exopolymer-producing halophilic luminescent bacteria were isolated from water samples collected from sampling sites of the rivers Mandovi and Zuari estuarine network connecting the coastal regions of Goa [40]. Among the screened isolates, the halophilic luminescent Vibrio harveyi strain VB23 showed the ability to form a viscous exopolymer possessing a good emulsifying activity.

The physicochemical properties of bioadhesives produced by a marine biofouling bacterium, Vibrio alginolyticus, were described by Muralidharan and Jayachandran [41]. According to gas chromatography/mass spectrometry (GC/MS) analysis, this EPS was formed by glucose, xylose, aminoribose and aminoarabinose with a molar ratio of 2:1:9:1. Indeed, the exopolysaccharide released by V. fischeri was composed by glucose, mannose, galactose, rhamnose and arabinose with a molar ratio of 3.4:3.7:1.5:0.6:0.7 [42].

Shewanella colwelliana, a marine microorganism that lives in association with oysters, synthesized an atypical EPS involved with the irreversible adhesion process of the bacterium to substrates. Furthermore, the production of the exopolymer was improved by growing this bacterium on marine agar. The purified exopolymer showed the presence of Ca, S, P and Si (40%–45%), carbohydrates (15%–35%), lipids (10%), and proteins (<5%) with glucose being the most abundant component of the carbohydrate moiety [43].

A potential hydrocarbon tolerance of Rhodococcus erythropolis PR4 was ascribed to two acidic EPSs (FR1 and FR2) produced by this marine bacterium. In particular FR2 was found to be composed of d-galactose, d-glucose, d-mannose, pyruvic acid and d-glucuronic acid, and also contained stearic and palmitic acids attached via ester bonds [44] to the sugar backbone.

Recently, several extremophilic microorganisms isolated from extreme environments (deep sea hydrothermal vents, Arctic and Antarctic ecosystems, saline lakes, geothermal springs, etc.), have been studied as potential sources of valuable EPSs in attempt to find new biopolymers with unique properties [3,23]. Since extremophiles offer important insights into biology and evolution studies, they could be considered as a valuable resource for exploitation in novel biotechnological processes. During the last decades, several reports have stated the production of EPSs produced by extremophilic microorganisms. These EPSs have been deeply investigated because of their widely diversified structure, biosynthesis, composition and functional properties even if only few of them have been used for industrial scopes. Nevertheless, the extremophilic microorganisms and their exopolysaccharides could find various biotechnological applications, thanks to some advantageous features like for example a short duration of fermentative processes in the case of thermophilic bacteria or an effortless production of stable emulsions of EPSs in the case of psychrophiles [26].

In the Archaea Domain a valuable source of EPS is embodied by bacteria isolated from salt lakes, volcanic and hydrothermal marine areas, like for example species of the genera Methanosarcina, Haloferax, Haloarcula, Thermococcus and Sulfolobus; Thermococcus litoralis and Archaeoglobus fulgidus in particular produced a peculiar biofilm composed of a consortium of cells immobilized inside an exopolymer, which may contribute to concentrating nutrients [45]. It is noteworthy that the first reported exopolymer was secreted by the halophilic archaebacterium Haloferax mediterranei, which was isolated from the Mediterrean Sea [46,47]. During the fermentation process in static conditions, the cells were found to be enveloped by an amorphous matrix. Notwithstanding, the growth conditions seemed to not affect the production of the polymer, and the extent of the cell aggregation in unshaken cultures appeared to be influenced by the presence of glucose. The analysis of EPSs in terms of rheological properties showed a pseudo plastic behavior coupled to an elevated apparent viscosity, which increased with the EPS concentration, even if the viscosity value was constant in all the studied conditions of pH, temperature and salinity. This polysaccharide together with its producing microorganism could represent a valuable candidate for the recovery of oil, especially in oil deposits with high saline concentrations.

Another Archaea EPS producer is the heterotrophic facultative sulfur-dependent hyperthermophilic Thermococcus litoralis which was able to synthesize exopolymers in a sulfur-free defined medium with a growth performance similar to that registered on complex media [48]. This microorganism, isolated from a shallow submarine thermal spring, has an optimal temperature of growth of 88 °C. The exopolysaccharide from T. litoralis displayed an unusual structure since it was formed by mannose that normally is found as a monomer sugar in polysaccharides from plants or yeasts. Moreover, 1% to 2% sulfate and 1.5% to 4.5% phosphorus substituents were also found in T. litoralis EPS.

In the Bacteria Domain, some marine thermophilic bacilli species have been reported as EPS producers, for example the Bacillus thermodenitrificans strain B3-72. The B. licheniformis strain B3-15, isolated from hot marine shallow vents of Vulcano island (Italy), is able to produce interesting EPSs that show antiviral activities [49,50]. The B. licheniformis strain T4 isolated from the Panarea island (Italy) is able to produce a fructo-fucan polymer that has an anti-citotoxic activity [51]. G. tepidamans V264, isolated from a Velingrad Bulgarian hot spring, is able to produce an unusually thermostable glucan [52]. And finally, Aeribacillus pallidus 418, isolated from the Bulgarian Rupi hydrothermal springs, is responsible for the synthesis of two novel EPSs [53].

Lin et al. [54] characterized the primary structure of a novel exopolysaccharide TA-1 secreted by Thermus aquaticus YT-1 that shows immune modulatory effects in murine macrophage and in human monocyte cell lines.

Among the extremophilic microorganisms, the halophiles represent the community that tolerates and/or requires high salt concentrations for their growth and that are widely demanded by several industrial sectors for their novel enzymatic activities and products with several possible applications [55]. In the Haloferax, Halobacterium, Natronococcus, Halococcus, and Haloarcula genera, many microorganisms are present that are able to produce EPSs. Considering the Halomonas genus, the species H. maura, H. eurihalina, H. ventosae, H. anticariensis and H. alkaliantarctica isolated from hypersaline environments, were shown to be good EPS producing species [56,57,58,59,60,61,62,63,64]. Typically the exopolysaccharides from Halomonas strains are characterized by a high presence of sulfate groups and uronic acids responsible for their gellifying actions.

4. EPS Production and Recovery

The improvement of production relies on fermentation techniques involving new strategies like the use of genetically engineered microorganisms and new methodologies, which result in high yield and cost-effective production of these biopolymers. The commercial exploitation of the biochemical microbial diversity has resulted in the development of the fermentation industry. Moreover, the new techniques of genetic manipulation have given the opportunity to develop new processes and to improve old ones [65]. The recovery of EPS, i.e., the “downstream processing”, requires the classical steps of the recovery of the product from the fermentation broth after the removal of insolubles (for example cells) by centrifugation, followed by isolation and purification steps. However, the EPS-producing cultures represent a challenge for the culture producers because of the high viscosity of the fermented growth media that makes the separation of the cells by centrifugation very difficult, which in turn results in serious problems related to heat transfer and oxygen supply [65]. In this case, a fed-batch culture is suitable to bypass highly viscous broths, even, as in the case of thermophilic EPS producers, the high temperature utilized for the growth of microorganisms can solve the problem.

At the end of the fermentation processes, the EPS can be recovered from the growth medium by separating the cells by centrifugation. Subsequently, the exopolysaccharides present in the cell-free medium are precipitated using ethanol or acetone or methanol. In a next step, the pellets that are recovered by centrifugation, go on to appropriate dialysis in distilled water, and are then freeze dried in order to achieve the crude EPS.

The limit of bacterial EPSs for industrial use can be ascribed to the scarce extent of their yields even if there are some strains of Xanthomonas campestris, Bacillus polymyxa, Klebsiella pneumonie and Sfingomonas elodea, for example, that are known for their high levels of biopolymer production [66,67,68,69,70].

Since the microbial EPSs possess different sugar compositions and different rheological characteristics, they represent a very big potential reserve within which it is possible to find the ideal EPS to use in a specific biotechnological application.

5. Fermentation Strategies

5.1. Effect of the Chemical Composition of the Medium and the Physical Parameters of Growth Conditions

The exopolysaccharide yields and the rheological aspects of these polymers depend on several critical factors related to fermentation conditions: carbon and nitrogen source utilization, mineral requirements, temperature and optimal pH but also agitation rate and oxygen consumption, just to give some examples (Table 1). From the literature, it is possible to assert that the nutritional and environmental conditions (culture conditions) can affect the yield and quality of microbial exopolysaccharides, whereas the prediction of molecular mass, number of monosaccharide units and degree of branching of EPS is possible by using a physiological control [9]. The nutrient limitation in marine bacteria (such as nitrogen, phosphorus, sulfur and potassium) can cause an increase in EPS production as stated by Sutherland [16]. Moreover, by setting several physical stressing factors, such as temperature, osmotic stress or others responsible for decreased growth, the EPS production may be enhanced. Furthermore, the selection of a most suitable carbon source for the growth medium composition represents the right effort to optimize the polymer production [23].

In recent times, Marx et al. [71] investigated the influence of temperature, salinity and pressure on EPS production in the psychrophilic gamma-proteobacterium Colwellia psychrerythraea strain 34H isolated from Arctic marine sediments. The authors noticed that the stressful environmental conditions increased EPS production; indeed in a range of temperatures between −8 °C to −14 °C, the EPS yield rose significantly. Similarly, higher pressures (400–600 atm) as well as higher salinity (10–100 parts per million, at the temperatures of −1 °C and −5 °C) significantly improved the production of EPS.

Mancuso et al. [72] described the effects of incubation temperature on growth and production of EPS by Antarctic sea ice bacterium grown in batch culture. In particular, when the strain CAM025 (member of the genus Pseudoalteromonas) was grown at −2 °C and 10 °C, the yields of EPS were 30 times higher than those at 20 °C, confirming the hypothesis of the cryoprotective role of EPS in the case of extremely low temperatures. Moreover, the EPS produced at −2 °C and 10 °C had a higher uronic acid content than that produced at 20 °C.

The effect of the growth temperature on the production of an exopolysaccharide named EPS-R [73] by the marine microorganism Hahella chejuensis, collected in Cheju Island, was studied as well. The highest productivity was obtained in the 20 to 25 °C temperature range while above 30 °C, productivity was reduced. In this study, other parameters were considered in order to optimize the production of EPS: In particular the authors noticed that among the nitrogen sources tested, tryptone provided the highest production level while among the carbon sources, sucrose was the best. In both cases, the best productivity (EPS/dried cell weight) was achieved with a sucrose/tryptone ratio of 2:1. The effects of NaCl, MgSO4 and CaCl2 on EPS production was also noticeable: These salts that were all required for the growth of this microorganism caused the highest accumulation of polymers when they were added to the media at 1%, 0.5% and 0.01% w/w, respectively.

Al-Nahas et al. [74] described the characterization of an EPS producing bacterium, named Pseudoalteromonas sp. AM, isolated from a sponge sample at about 16 m depth in the Red Sea (Hurghada, Egypt). The production of this EPS was achieved by fermentation in 250 mL shake flasks containing 50 mL of casein hydrolysate-glucose broth at 30 °C. The effect of different carbon sources including galactose, fructose, lactose, sucrose, dextrin, glycerol, molasses and citric acid, was tested. In addition, different nitrogen sources such as meat extract, yeast extract, tryptone, peptone, ammonium sulfate, ammonium oxalate and sodium nitrate were also tested. The results showed that the maximum EPS productivity was achieved after 7 days at pH 7, at an agitation of 150 rpm in a fermentation medium containing glucose, meat extract and 3% NaCl.

Recently, a novel bacterium strain BM39, affiliated with Pantoea sp., isolated from sediments collected in the Tyrrhenian Sea, was selected for its ability to produce very high levels of glucan EPS [66]. Kinetic studies of EPS production by strain BM39 cultivated in shaken cultures on different media indicated that the maximum EPS production (21.30 ± 2.03 g/L) was obtained in EMG medium (containing glucose 80 g/L as carbon source) with a maximum of EPS time productivity of 0.89 ± 0.09 g/Lh; using a medium containing 80 g/L of sucrose (EMS medium) or 80.0 g/L of fructose (EMF medium) as carbon sources, the EPS productions registered were 11.82 ± 1.06 g/L and 11.05 ± 1.17 g/L, respectively, while the productivity was 0.39 ± 0.04 g/Lh and 0.37 ± 0.04 g/Lh, respectively.

The effect of carbon sources was also studied in Zunongwangia profunda SM-A87: The maximum EPS production, about 6.47 g/L, was detected when lactose was added to the basic marine medium with the other carbon sources tested being glucose, mannose, maltose and sucrose [75].

The polysaccharide 1644 produced by a strain of Alteromonas sp. showed a unique rheological behavior [76]. The purified EPS, in the presence of divalent ions, formed an elastic gel, which can be stretched reversibly without any loss of structure [36]. Dubreucq et al. [77] clarified its structure indicating the presence of an unusual dicarboxylic acid sugar in the repeating unit, probably responsible for the high affinity of this polymer for divalent ions. In contrast to some other bacterial EPSs, which are synthesized during active bacterial growth, the polysaccharide 1644 is produced only during the initial exponential growth phase. In order to improve its production, Saiman et al. [76] checked the use of a mineral-defined medium containing ammonium chloride as sole nitrogen source instead of peptone and yeast extract. The fermentation strategy started with an ammonium chloride concentration of 0.4 g/L. When the microorganism reached the initial exponential phase, the ammonium chloride level was kept continually low, but the concentration was enough in order to permit protein synthesis. The synthesis of EPS was continuous during the nitrogen source use and persisted linearly up to the conclusion of the fermentation, generating EPS yields 50% higher than those obtained with the complex medium.

Llamas et al. [31] studied the heteropolysaccharide produced by the strain of Salipiger mucosus A3T, a halophilic species belonging to the Alphaproteobacteria genus and isolated from the Spanish Mediterranean seaboard. The kinetics of its production illustrated that the polymer was synthesized essentially during the exponential phase but persisted during the stationary phase with a lower yield. EPS was excreted mainly during the exponential growth phase but continued to a lesser extent during the stationary phase reaching the value of 120 mg EPS/100 mL broth. Moreover, EPS yield was always related to the quantity of biomass in culture and the EPS production was best at a 2.5% salt concentration. As far as incubation temperature was concerned, EPS and cell growth yields were lower at both 22 °C and 42 °C than at 32 °C. Similar results were achieved when the pH value of the medium was lower or higher than 7.0. The same trend was also obtained for both static incubation or at a stirring rate of more than 100 rpm, causing comparably lower growth and lower EPS yields [31].

In the hyperthermophilic Thermococcus litoralis, the EPS production was significantly stimulated by adding NH4Cl in continuous culture at high dilution rates: The EPS, acting as a transporter of reducing equivalents out of the cell, allows the microorganism’s survival [78]. Another Archaea that secretes exopolysaccharides as a defense mechanism when exposed to stress is Archaeglobus fulgidus, an anaerobic marine hyperthermophile [79]. Studies of biofilm production showed that the biofilm secretion was stimulated by exposure of the microorganism to stress factors, such as pH and temperature, or high concentrations of antimicrobial agents.

The effect of carbon sources was also studied in Aeribacillus pallidus 418 [53] in which a basal medium supplemented with maltose (0.9%) gave the best EPS and biomass production, of 80 μg/mL and 0.75 mg/mL, respectively. Moreover, regarding the nitrogen source, the highest EPS production was observed when ammonium salts (0.2%) were added to the basal medium, while organic sources provided a better growth. Regarding the effects of temperature (between 50 and 70 °C with 5 °C temperature steps) and pH value (between 6.0 and 8.5 with 0.5 pH steps) on EPS synthesis, the highest polymer production was observed at 55 °C and pH 7.0.

As reported until now, the abundance and the structure of polysaccharides are mainly affected by the culture medium composition. Usually sugars are found as the preferred carbon source to synthesize such exopolymers. Indeed, the haloalkalophilic Halomonas alkaliantarctica strain CRSS produces two different exopolysaccharides, a mannan or a xylo-mannan type glycan, when cells are grown on two different complex media, while a different polysaccharide with higher yield, a fructo-glucan type, is released in the presence of sodium acetate as sole carbon source in the minimal medium [64]. Additionally, thermophilic bacteria showing mucous colonies and belonging to Bacillus-Thermus genera have been isolated from shallow, marine hydrothermal vents of the flegrean area in Italy and have been characterized as EPS producers [80]. Among the different strains isolated, the strain 4009 collected in Ischia (Sorceto) island, reached an EPS yield of 60 mg/L using trehalose as sole carbon source, a value that was about 1000-fold compared to the minimal medium.

Table 1. Examples of fermentation strategies for EPS production in marine microorganisms.
Table 1. Examples of fermentation strategies for EPS production in marine microorganisms.
MicroorganismsSourceMax EPS-productionEPS Fermentation-increasing strategiesProduction increment (fold)References
Aeribacillus pallidus 418Hot springs Bulgaria0.13 g/LCarbon and nitrogen sources: maltose, NH4Cl; temperature2Radchenkova et al., 2013 [53]
Alteromonas sp. 1644Hydrothermal vents East Pacific Rise7.5 g/LNitrogen source: ammonium chloride1.5Samain et al., 1997 [76]
Hahella chejuensisCheju Island9.23 g/LCarbon/nitrogen ratio: sucrose, tryptone; temperature, pHn.r.Sung-Hwan Ko et al., 2000 [73]
Halomonas alkaliantarctica strain CRSSCape Russell lake, Antarctica2.9 g/g dry cellsCarbon source: maltose6Poli et al., 2004 [64]
Pantoea strain BM39Sediments in Tyrrhenian Sea21.30 g/LCarbon source: glucose2Silvi et al., 2013 [66]
Pseudoalteromonas sp. AMSponge sample in Red Sea10.51 g/LCarbon and nitrogen sources: meat extract, glucose; NaCl; pH; agitation speed5Al-Nahas et al., 2011 [74]
Pseudoalteromonas strain CAM025Antarctic sea ice99.9 mg/g dry cellsTemperature30Mancuso et al., 2005 [72]
Salipiger mucosus A3TSpanish Mediterranean seaboard1.2 g/LStirring rate; incubation temperature; pHn.r.Llamas et al., (2010) [31]
Thermophilic bacterium strain 4009Ischia (Sorceto) Island60 mg/LCarbon sources: trehalose1000Nicolaus et al., 2002 [80]
Zunongwangia profunda SM-A87Deep-sea sediment southern Okinawa Trough8.90 g/LCarbon and nitrogen sources: lactose, peptone; temperature; statistical approach10Liu et al., 2011 [75]

n.r.: Not reported.

5.2. Alternative Cheap Sources for EPS Production

Most of the costs related to the achievement of EPSs in industrial processes are due to the media composition. Sugars are the common substrates utilized during the microbial fermentation to produce EPSs. Nowadays, there are several reports that describe the formation of exopolymers using alternative and cheaper carbon sources, such as industrial residual materials, agro wastes, etc. This new slant, if producing good results, is to be preferred, because it represents an opportunity to produce valuable substances like exopolysaccharides with a wide range of biotechnological applications using cheaper substrates, and at the same time to contribute to waste disposal, which is an expensive process in itself.

More et al. [81] described the isolation from wastewater sludge of thirteen EPS-producing bacterial strains that belong to the Bacillus, Serratia and Yersina genera. All the isolated strains showed the ability to synthesize extracellular polymeric substances, even when using secondary wastewater sludge (without chemical polymers) as the growth media.

For the soil isolate Bacillus subtilis, agro substrates, cane molasses, and rice bran in different concentrations were tested to enhance the EPS production with respect to sucrose; cane molasses at a concentration of 2% lead to the highest yield of 4.86 g/L compared to a medium with sucrose (2.98 g/L) as sole carbon source [82]. Küçükaşik and co-workers [83] also tested pretreated sugar beet molasses and starch molasses as carbon sources for levan production by the Halomonas smyrniensis strain AAD6, and both substrates resulted in working alternatives to sucrose. In particular, when using 50 g/L of sucrose in the growth medium, the levan yield was 1.84 g/L, whereas in the presence of 30 g/L of sugar beet molasses as sole carbon source, the achieved levan production was 12.4 g/L. The soil isolate levan producer Bacillus polymyxa (NRRL-18475) was found to be able to synthesize the EPS using appropriately modified sugarcane juice and beet molasses with a satisfactory yield [84]. A molasses-based medium has been demonstrated to also be suitable for gellan gum production by Sphingomonas paucimobilis ATCC-31461 [85]. Sugar beet molasses used as sole carbon source was also shown to be suitable for xanthan gum fermentation by Xanthomonas campestris ATCC 1395 [86].

In the literature, there is no study concerning the improvement of the EPS production process by marine bacteria; nevertheless it would also be interesting to investigate the potentiality of these microorganisms to secrete EPS utilizing alternative carbon sources.

5.3. Statistical Tools

The microbial exopolysaccharides are fermentation products the yield, composition and, therefore, properties of which are the result of the combination of numerous variables, as explained in this review. Clearly, to reach the best fermentative conditions, several experiments must be done and several hypotheses must be developed, without any outcome warranty and with expenditure of chemicals, time and energy. Increasingly, statistical approaches are also being propagated in the field of EPS production. Their use provides an immediate instrument to individuate the suitable parameters to be modified and to decide in which direction to go in order to obtain with high probability what research is interested in. This way, the number of experiments can be drastically reduced, as they are more specifically focused. In the literature, Plackett-Burman (PB) design and response surface methodologies (RSM) are the most common approaches reported for the optimization of the EPS production process. The PB experimental design [87] is a valuable tool generally used to screen main factors from a number of process variables. The RSM is an efficient statistical strategy widely selected to improve product yields and to reduce overall process time and costs; it is suitable for planning experiments and predicting the optimal conditions of parameters involved in a process [75]. Qiang et al. [88] used RSM for EPS production by Klebsiella sp. H-207, isolated from activated sludge. A maximum polysaccharide yield of about 15.05 g/L was achieved under optimized conditions in terms of both medium composition and culture conditions, which consisted of sucrose 31.93 g/L, KNO3 2.17 g/L and K2HPO4 5.47 g/L, a seed age of 13 h, with an inoculum size of 10.6% and an incubation temperature of 28.9 °C. Zunongwangia profunda SM-A87 isolated from deep-sea sediment, is the first marine bacterium that produces EPS with the high yield of 8.90 g/L. On the basis of this result there is an RSM approach that is used to select the more sensitive variables with respect to the study objective and results in the necessary amount of lactose and peptone and the incubation time [75].

Screening of the most significant fermentation parameters affecting levan production was done by the PB design for the microbial strain Pseudomonas fluorescens NCIM 2059. Six nutritional variables (sucrose, casein peptone, NH4Cl, KH2PO4, MgSO4, and NaNO3) were studied to define the optimal medium. A significant increase of levan yield from 5.27 up to 15.42 g/L under these conditions was found [89].

5.4. Genetic Approach

The exopolysaccharide production is a genetically determined process. Hence, in order to improve the microbial EPS synthesis, an accurate approach should first identify all the genes responsible for polymer synthesis and then try to comprehend the mechanisms involved. This represents what science has been doing in the last decade, giving more and more privilege to studies on a genomic level.

Effectively, once a complete view of a microbial EPS-producing genome has been obtained, it is possible to choose the right strategy to improve the polymer release through manipulation of the genes encoding the enzymes involved in the biosynthesis, or by altering the regulatory pathways that affect gene expression and enzyme activity, as well as by selecting the most suitable substrate to be supplied to the microorganism during growth.

To our knowledge, in the field of marine EPS-producing bacteria, the performed genomic studies have provided clear indications only regarding the adaptation and evolution mechanisms needed to survive in determinate environmental growth conditions, hence attributing a relevant ecological role to the exopolysaccharides [30].

Zunongwangia profunda SM-A87, as many other deep-sea isolates, produces large quantities of exopolysaccharide [75]. Its genome was the first sequenced in the phylum of Bacteroidetes [90]. Apart from various extracellular enzymes for carbohydrate, lipid and DNA degradation, it possesses two polysaccharide biosynthesis gene clusters. Its genome analysis reveals the presence of some common features of deep-sea bacteria.

The deep-sea psychrotolerant gammaproteobacterium Pseudoalteromonas sp. SM9913 also produces large quantities of EPS [28]. This EPS was able to enhance the stability of the cold-adapted protease MCP-01 secreted by the same strain through preventing its autolysis. In addition, an ecological role connected to the adaptation to the deep-sea ecosystem was attributed to the purified EPS. The Pseudoalteromonas sp. SM9913 genome was sequenced, and a comparative study with the closely related Antarctic surface sea-water ecotype Pseudoalteromonas haloplanktis TAC125 (TAC125) was performed by Qin et al. [91]. Some deep-sea bacteria the genomes of which have been sequenced, such as Idiomarina loihiensis [92] and Alteromonas macleodii “deep ecotype” [93], present EPS biosynthesis genes, thus confirming that the production of EPS may be a common strategy that deep-sea bacteria adopt to endure extreme conditions.

Even if, to our knowledge, there are no cases of marine bacteria whose genome sequence analysis has been used to increase the exopolysaccharide yield, it would be desirable to extend this approach to these microorganisms in the near future.

On the contrary, in the case of the halophilic Halomonas smyrniensis strain AAD6 levan producer, the knowledge of the genome reconstruction (first performed using the microorganisms Chromohalobacter salexigens DSM 3043 that is taxonomically close to H. smyrniensis [21], and then from the whole-genome sequence) allowed the prediction of the stimulatory effect of mannitol on levan biosynthesis, which was later experimentally confirmed by Ates et al. [22]. Several other metabolic engineering efforts to improving production of sugar polymers have been attempted; for instance for the production of the following EPS: xanthan [94], gellan [23], cellulose [95] and levan [94]. Not all attempts have been successful; indeed only for cellulose was an increase polymer yield obtained [94,95]. Unfortunately, in the other cases, the results were not as encouraging, most probably because it would be necessary to get a deeper insight into both the single steps and the overall regulation of the pathways [23,94].

6. Conclusions

Although diverse microbial exopolysaccharides have been studied in the last years, only little information is available regarding their hyperproduction. In order to improve the fermentation processes of bacterial EPS, it is possible to operate at different levels, by searching for the ideal nutritional conditions resulting in the greatest yield of EPS with more suitable biotechnological proprieties, as well as by operating at the genomic level by inserting or finding those genes that are directly involved in sugar metabolism (Figure 1). Both strategies, possibly also applied together, can lead to promising results as a consequence of an interdisciplinary approach based on the analysis of complex system biological interactions and supported by statistical tools and predictive studies.

Figure 1. Examples of marine exopolysaccharides (EPS) producers and improvement strategies for EPS production. (A) “Secca Fumosa” located in the Gulf of Pozzuoli, Naples, Italy, taken by Dr. Guido Villani; (B) Samples collected by Dr. Annarita Poli in the “Cape Russell” lake in the Ross Sea, Antarctica (74 52.35 S 163 53.03 E) during the XXI Italian Antarctica Expedition.
Figure 1. Examples of marine exopolysaccharides (EPS) producers and improvement strategies for EPS production. (A) “Secca Fumosa” located in the Gulf of Pozzuoli, Naples, Italy, taken by Dr. Guido Villani; (B) Samples collected by Dr. Annarita Poli in the “Cape Russell” lake in the Ross Sea, Antarctica (74 52.35 S 163 53.03 E) during the XXI Italian Antarctica Expedition.
Marinedrugs 12 03005 g001 1024


The authors thank Guido Villani of CNR-ICB for the picture of “Secca Fumosa” in the Gulf of Pozzuoli, Naples, Italy, and the “First executive programme of the agreement between the government of the republic of Italy and the government of the republic of Turkey on scientific and technical cooperation”, entitled: “Extremophiles for next-generation biofuels” (MAE-TUBITAK No. M00192).

Author Contributions

All the authors contributed to the writing of the manuscript. They jointly developed the structure and arguments for the paper. All the authors reviewed and approved the final manuscript.

Conflicts of Interest

The authors declare no conflict of interest.


  1. Sponga, F.; Cavaletti, L.; Lazzarini, A.; Borghi, A.; Ciciliato, I.; Losi, D.; Marinelli, F. Biodiversity and potentials of marine-derived microorganisms. J. Biotechnol. 1999, 70, 65–69. [Google Scholar] [CrossRef]
  2. Mancuso Nichols, C.A.; Guezennec, J.; Bowman, J.P. Bacterial Exopolysaccharides from Extreme Marine Environments with Special Consideration of the Southern Ocean, Sea Ice, and Deep-Sea Hydrothermal Vents: A Review. Mar. Biotechnol. 2005, 7, 253–271. [Google Scholar] [CrossRef]
  3. Poli, A.; Anzelmo, G.; Nicolaus, B. Bacterial Exopolysaccharides from Extreme Marine Habitats: Production, Characterization and Biological Activities. Mar. Drugs 2010, 8, 1779–1802. [Google Scholar] [CrossRef]
  4. Zanchetta, P.; Lagarde, N.; Guezennec, J. A new bone-healing material: A hyaluronic acid-like bacterial exopolysaccharide. Calcif. Tissue Int. 2003, 72, 74–79. [Google Scholar]
  5. Mansel, P.W.A. Polysaccharides in skin care. Cosmet. Toilet. 1994, 109, 67–72. [Google Scholar]
  6. Satpute, S.K.; Banat, I.M.; Dhakephalkar, P.K.; Banpurkar, A.G.; Chopade, B.A. Biosurfactants, bioemulsifiers and exopolysaccharides from marine microorganisms. Biotechnology 2010, 28, 436–450. [Google Scholar]
  7. Chu, K.H.; Kim, E.Y. Predictive modelling of competitive biosorption equilibrium data. Biotechnol. Bioprocess Eng. 2006, 11, 67–71. [Google Scholar]
  8. Santhiya, D.; Subramanian, S.; Natarajan, K.A. Surface chemical studies on sphalerite and galena using extracellular polysaccharides isolated from Bacillus polymyxa. J. Colloid Interface Sci. 2002, 256, 237–248. [Google Scholar] [CrossRef]
  9. Kumar, A.S.; Mody, K.; Jha, B. Bacterial exopolysaccharides: A perception. J. Basic Microbiol. 2007, 47, 103–117. [Google Scholar] [CrossRef]
  10. Donot, F.; Fontana, A.; Baccou, J.C.; Schorr-Galindo, S. Microbial exopolysaccharides: Main examples of synthesis, excretion, genetics and extraction. Carbohydr. Polym. 2012, 87, 951–962. [Google Scholar] [CrossRef]
  11. Decho, A.W. Microbial exopolymer secretions in ocean environments: Their role(s) in food webs and marine processes. In Oceanography and Marine Biology: An Annual Review; Barnes, H., Ed.; Aberdeen University Press: Aberdeen, UK, 1990; pp. 73–153. [Google Scholar]
  12. Kenne, L.; Lindberg, B. Bacterial polysaccharides. In The Polysaccharides; Aspinall, G.O., Ed.; Academic Press: New York, NY, USA, 1983; Volume 2, pp. 287–363. [Google Scholar]
  13. Sutherland, I.W. Microbial exopolysaccharide synthesis. In Extracellular Microbial Polysaccharides; Sanford, P.A., Laskin, A., Eds.; American Chemical Society: Washington, DC, USA, 1977; Volume 45, pp. 40–57. [Google Scholar]
  14. Sutherland, I.W. Structure-function relationship in microbial exopolysaccharides. Biotechnol. Adv. 1994, 12, 393–448. [Google Scholar] [CrossRef]
  15. Vandamme, E.; de Baets, S.; Steinbuchel, A. Biopolymers: Polysaccharides I—Polysaccharides from Prokaryotes; Wiley-VCH Verlag GmbH: Weinheim, Germany, 2002. [Google Scholar]
  16. Sutherland, I.W. Biosynthesis of microbial exopolysaccharides. Adv. Appl. Microbiol. 1982, 23, 79–150. [Google Scholar]
  17. Wolfaardt, G.M.; Lawrence, J.R.; Korbe, D.R. Function of EPS. In Microbial Extracellular Polymeric Substances: Characterization, Structure and Function; Wingender, J., Neu, T.R., Flemming, H.-C., Eds.; Springer-Verlag: New York, NY, USA, 1999; pp. 171–200. [Google Scholar]
  18. Remminghorst, U.; Rehm, B.H.A. Microbial production of alginate: Biosynthesis and applications. In Microbial Production of Biopolymers and Polymer Precursor: Applications and Perspectives; Caister Academic Press: Palmerston North, New Zealand, 2009. [Google Scholar]
  19. Grobben, G.J.; Smith, M.R.; Sikkema, J.; de Bont, J.A. Influence of fructose and glucose on the production of exopolysaccharides and the activities of enzymes involved in the sugar metabolism and the synthesis of sugar nucleotides in Lactococcus delbrueckii subsp. bulgaricus NCFB 2772. Appl. Microbiol. Biotechnol. 1996, 46, 279–284. [Google Scholar] [CrossRef]
  20. Laws, A.; Gu, Y.; Marshall, V. Biosynthesis, characterisation, and design of bacterial exopolysaccharides from lactic acid bacteria. Biotechnol. Adv. 2001, 19, 597–625. [Google Scholar] [CrossRef]
  21. Ateş, Ö.; Toksoy, E.O.; Arga, K.Y. Genome-scale Reconstruction of Metabolic Network for a Halophilic Extremophile, Chromohalobacter salexigens DSM 3043. BMC Syst. Biol. 2011, 5. [Google Scholar] [CrossRef]
  22. Ateş, Ö.; Arga, K.Y.; Öner, E.O. The stimulatory effect of mannitol on levan biosynthesis: Lessons from metabolic systems analysis of Halomonas smyrnensis AAD6T. Biotechnol. Progress 2013, 29, 1386–1397. [Google Scholar] [CrossRef]
  23. Nicolaus, B.; Kambourova, M.; Toksoy, E.O. Exopolysaccharides from extremophiles: From fundamentals to biotechnology. Environ. Technol. 2010, 31, 1145–1158. [Google Scholar] [CrossRef]
  24. Fenical, W. Chemical studies of marine bacteria: Developing a new resource. Chem. Rev. 1993, 93, 1673–1683. [Google Scholar] [CrossRef]
  25. Iyer, A.; Mody, K.; Jha, B. Characterization of an exopolysaccharide produced by a marine Enterobacter cloacae. Indian J. Exp. Biol. 2005, 43, 467–471. [Google Scholar]
  26. Mancuso Nichols, C.A.; Garon, S.; Bowman, J.P.; Raguénès, G.; Guézennec, J. Production of exopolysaccharides by Antarctic marine bacterial isolates. J. Appl. Microbiol. 2004, 96, 1057–1066. [Google Scholar]
  27. Rougeaux, H.; Guezennec, J.; Carlson, R.W.; Kervarec, N.; Pichon, R.; Talaga, P. Structural determination of the exopolysaccharide of Pseudoalteromonas strain HYD 721 isolated from a deep-sea hydrothermal vent. Carbohydr. Res. 1999, 315, 273–285. [Google Scholar] [CrossRef]
  28. Qin, K.; Zhu, L.; Chen, L.; Wang, P.G.; Zhang, Y. Structural characterization and ecological roles of a novel exopolysaccharide from the deep-sea psychrotolerant bacterium Pseudoalteromonas sp. SM9913. Microbiology 2007, 153, 1566–1572. [Google Scholar] [CrossRef]
  29. Li, W.W.; Zhou, W.Z.; Zhang, Y.Z.; Wang, J.; Zhu, X.B. Flocculation behavior and mechanism of an exopolysaccharide from the deep-sea psychrophilic bacterium Pseudoalteromonas sp. SM9913. Bioresour. Technol. 2008, 99, 6893–6899. [Google Scholar]
  30. Liu, S.B.; Chen, X.L.; He, H.L; Zhang, X.Y.; Xie, B.B.; Yu, Y.; Chen, B.; Zhou, B.C.; Zhang, Y.Z. Structure and Ecological Roles of a Novel Exopolysaccharide from the Arctic Sea Ice Bacterium Pseudoalteromonas sp. Strain SM20310. Appl. Environ. Microbiol. 2013, 79, 224–230. [Google Scholar] [CrossRef]
  31. Llamas, I.; Mata, J.A.; Tallon, R.; Bressollier, P.; Urdaci, M.C.; Quesada, E.; Béjar, V. Characterization of the Exopolysaccharide Produced by Salipiger mucosus A3T, a Halophilic Species Belonging to the Alphaproteobacteria, Isolated on the Spanish Mediterranean Seaboard. Mar. Drugs 2010, 8, 2240–2251. [Google Scholar]
  32. Vincent, P.; Pignet, P.; Talmont, F.; Bozzi, L.; Fournet, B.; Guezennec, J.; Jeanthon, C.; Prieur, D. Production and characterization of an hydrothermal vent bacterium isolated from the polychaete annelid exopolysaccharide excreted by a deep-sea Alvinella pompejana. Appl. Environ. Microbiol. 1994, 60, 4134–4141. [Google Scholar]
  33. Rougeaux, H.; Talaga, P.; Carlson, R.W.; Guerzennec, J. Structural studies of an exopolysaccharide produced by Alteromonas macleodii subsp. fijiensis originating from a deep-sea hydrothermal vent. Carbohydr. Res. 1998, 312, 53–59. [Google Scholar] [CrossRef]
  34. Zanchetta, P.; Guezennec, J. Surface thermodynamics of osteoblasts: Relation between hydrophobicity and bone active biomaterials. Colloids Surf. B 2001, 22, 301–307. [Google Scholar] [CrossRef]
  35. Colliec Jouault, S.; Chevolot, L.; Helley, D.; Ratiskol, J.; Bros, A.; Sinquin, C.; Roger, O.; Fischer, A.-M. Characterization, chemical modifications and in vitro anticoagulant properties of an exopolysaccharide produced by Alteromonas infernus. Biochim. Biophys. Acta 2001, 1528, 141–151. [Google Scholar]
  36. Bozzi, L.; Milas, M.; Rinaudo, M. Characterization and solution properties of a new exopolysaccharide excreted by the bacterium Alteromonas sp. strain 1644. Int. J. Biol. Macromol. 1996, 18, 9–17. [Google Scholar] [CrossRef]
  37. Bozzi, L.; Milas, M.; Rinaudo, M. Solution and gel rheology of a new exopolysaccharide excreted by the bacterium Alteromonas sp. strain 1644. Int. J. Biol. Macromol. 1996, 18, 83–91. [Google Scholar]
  38. Wrangstadh, M.; Szewzyk, U.; Ostling, J.; Kjelleberg, S. Starvation-Specific Formation of a Peripheral Exopolysaccharide by a Marine Pseudomonas sp., Strain S9. Appl. Environ. Microbiol. 1990, 56, 2065–2072. [Google Scholar]
  39. Lim, D.J.; Kim, J.D.; Kim, M.Y.; Yoo, S.H.; Kong, J.Y. Physicochemical Properties of the Exopolysaccharides Produced by Marine Bacterium Zoogloea sp. KCCM10036. J. Microbiol. Biotechnol. 2007, 17, 979–984. [Google Scholar]
  40. Bramhachari, P.V.; Dubey, S.K. Production and characterization of exopolysaccharide produced by Vibrio harveyi strain VB23. Lett. Appl. Microbiol. 2006, 43, 571–577. [Google Scholar] [CrossRef]
  41. Muralidharan, J.; Jayachandran, S. Physicochemical analyses of the exopolysaccharides produced by a marine biofouling bacterium, Vibrio alginolyticus. Process Biochem. 2003, 38, 841–847. [Google Scholar]
  42. Rodrigues, C.; Bhosle, N. Exopolysaccharide production by Vibrio fischeri, a fouling marine bacterium. Biofouling 1991, 4, 301–308. [Google Scholar]
  43. Abu, G.O.; Weiner, R.M.; Rice, J.; Colwell, R.R. Properties of an extracellular adhesive polymer from the marine bacterium, Shewanella colwelliana. Biofouling 1991, 3, 69–84. [Google Scholar] [CrossRef]
  44. Urai, M.; Yoshizaki, H.; Anzai, H.; Ogihara, J.; Iwabuchi, N.; Harayama, S.; Sunairi, M.; Nakajima, M. Structural analysis of mucoidan, an acidic extracellular polysaccharide produced by a pristane-assimilating marine bacterium, Rhodococcus erythropolis PR4. Carbohydr. Resour. 2007, 342, 927–932. [Google Scholar] [CrossRef]
  45. Poli, A.; di Donato, P.; Abbamondi, G.R.; Nicolaus, B. Synthesis, Production, and Biotechnological Application of Exopolysaccharides and Polyhydroxyalkanoates by Archaea. Archaea 2011, 2011. [Google Scholar] [CrossRef]
  46. Anton, J.; Meseguer, I.; Rodriguez-Valera, F. Production of an Extracellular Polysaccharide by Haloferax mediterranei. Appl. Environ. Microbiol. 1988, 10, 2381–2386. [Google Scholar]
  47. Parolis, H.; Parolis, L.A.S.; Boán, I.F.; Rodríguez-Valera, F.; Widmalm, G.; Manca, M.C.; Jansson, P.-E.; Sutherland, I.W. The structure of the exopolysaccharide produced by the halophilic Archaeon Haloferax mediterranei strain R4 (ATCC 33500). Carbohydr. Resour. 1996, 295, 147–156. [Google Scholar] [CrossRef]
  48. Rinker, K.D.; Kelly, R.M. Growth Physiology of the Hyperthermophilic Archaeon Thermococcus litoralis: Development of a Sulfur-Free Defined Medium, Characterization of an Exopolysaccharide, and Evidence of Biofilm Formation. Appl. Environ. Microbiol. 1996, 12, 4478–4485. [Google Scholar]
  49. Maugeri, T.L.; Gugliandolo, C.; Caccamo, D.; Panico, A.; Lama, L.; Gambacorta, A.; Nicolaus, B. A halophilic thermotolerant Bacillus isolated from a marine hot spring able to produce a new exopolysaccharide. Biotechnol. Lett. 2002, 24, 515–519. [Google Scholar]
  50. Arena, A.; Maugeri, T.L.; Pavone, B.; Iannello, D.; Gugliandolo, C.; Bisignano, G. Antiviral and immunoregulatory effect of a novel exopolysaccharide from a marine thermotollerant Bacillus licheniformis. Int. Immunopharmacol. 2006, 6, 8–13. [Google Scholar] [CrossRef]
  51. Spanò, A.; Gugliandolo, C.; Lentini, V.; Maugeri, T.L.; Anzelmo, G.; Poli, A.; Nicolaus, B. A novel EPS-producing strain of Bacillus licheniformis isolated from a shallow vent off Panarea Island (Italy). Curr. Microbiol. 2013, 67, 21–29. [Google Scholar]
  52. Kambourova, M.; Mandeva, R.; Dimova, D.; Poli, A.; Nicolaus, B.; Tommonaro, G. Production and characterization of a microbial glucan, synthesized by Geobacillus tepidamans V264 isolated from Bulgarian hot spring. Carbohydr. Polym. 2009, 77, 338–343. [Google Scholar] [CrossRef]
  53. Radchenkova, N.; Vassilev, S.; Panchev, I.; Anzelmo, G.; Tomova, I.; Nicolaus, B.; Kuncheva, M.; Petrov, K.; Kambourova, M. Production and properties of two novel exopolysaccharides synthesized by a thermophilic bacterium Aeribacillus pallidus 418. Appl. Biochem. Biotechnol. 2013, 171, 31–43. [Google Scholar]
  54. Lin, M.H.; Yang, Y.L.; Chen, Y.P.; Hua, K.F.; Lu, C.P.; Sheu, F.; Lin, G.H.; Tsay, S.S.; Liang, S.M.; Wu, S.H. A novel exopolysaccharide from the biofilm of Thermus aquaticus YT-1 induces the immune response through Toll-like receptor 2. J. Biol. Chem. 2011, 286, 17736–17745. [Google Scholar]
  55. Ventosa, A.; Nieto, J.J.; Oren, A. Biology of moderately halophilic aerobic bacteria. Microbiol. Mol. Biol. Rev. 1998, 62, 504–544. [Google Scholar]
  56. Bejar, V.; Llamas, I.; Calvo, C.; Quesada, E. Characterization of exopolysaccharides produced by 19 halophilic strains of the species Halomonas eurihalina. J. Biotechnol. 1998, 61, 135–141. [Google Scholar] [CrossRef]
  57. Arias, S.; del Moral, A.; Ferrer, M.R.; Tallon, R.; Quesada, E.; Béjar, V. Mauran, an exopolysaccharide produced by the halophilic bacterium Halomonas maura, with a novel composition and interesting properties for biotechnology. Extremophiles 2003, 7, 319–326. [Google Scholar] [CrossRef]
  58. Quesada, E.; Valderrama, M.J.; Béjar, V.; Ventosa, A.; Gutiérrez, M.C.; Ruiz-Berraquero, F.; Ramos-Cormenzana, A. Volcaniella eurihalina gen. nov., sp. nov., a moderately halophilic non motile gram-negative rod. Int. J. Syst. Evolut. Microbiol. 1990, 40, 261–267. [Google Scholar]
  59. Quesada, E.; Béjar, V.; Calvo, C. Exopolysaccharide production by Volcaniella eurihalina. Experientia 1993, 49, 1037–1041. [Google Scholar] [CrossRef]
  60. Quesada, E.; Béjar, V.; Del Moral, A.; Ferrer, M.R.; Calvo, C.; Llamas, I.; Martinez-Checa, F.; Arias, S.; Ruiz-Garcìa, C.; Martinez-Cánovas, J.; et al. Moderately halophilic exopolysaccharide-producing bacteria. In Halophilic Microorganisms; Ventosa, A., Ed.; Springer-Verlag: Heidelberg, Germany, 2004; pp. 297–314. [Google Scholar]
  61. Martínez-Cánovas, M.J.; Quesada, E.; Llamas, I.; Béjar, V. Halomonas ventosae sp. nov., a moderately halophilic, denitrifying, exopolysaccharide-producing bacterium. Int. J. Syst. Evolut. Microbiol. 2004, 54, 733–737. [Google Scholar] [CrossRef]
  62. Bouchotroch, S.; Quesada, E.; Izquierdo, I.; Rodriguez, M.; Béjar, V. Bacterial exopolysaccharide produced by newly discovered bacteria belonging to the genus Halomonas, isolated from hypersaline habitats in Morocco. J. Ind. Microbiol. Biotechnol. 2000, 24, 374–378. [Google Scholar] [CrossRef]
  63. Bouchotroch, S.; Quesada, E.; del Moral, A.; Llamas, I.; Bejar, V. Halomonas maura sp. nov. a novel moderately halophilic, exopolysaccharide-producing bacterium. Int. J. Syst. Evolut. Microbiol. 2001, 51, 1625–1632. [Google Scholar] [CrossRef]
  64. Poli, A.; Esposito, E.; Orlando, P.; Lama, L.; Giordano, A.; de Appolonia, F.; Nicolaus, B.; Gambacorta, A. Halomonas alkaliantarctica sp. nov., isolated from saline lake Cape Russell in Antarctica, an alkalophilic moderately halophilic, exopolysaccharide-producing bacterium. Syst. Appl. Microbiol. 2007, 30, 31–38. [Google Scholar] [CrossRef]
  65. Sameera, V. Novel techniques in the production of industrially imperative products. J. Microb. Biochem. Technol. 2011, R1. [Google Scholar] [CrossRef]
  66. Silvi, S.; Barghini, P.; Aquilanti, A.; Juarez-Jimenez, B.; Fenice, M. Physiologic and metabolic characterization of a new marine isolate (BM39) of Pantoea sp. producing high levels of exopolysaccharide. Microb. Cell Fact. 2013, 12. [Google Scholar] [CrossRef]
  67. Lee, I.Y.; Seo, W.T.; Kim, G.J.; Kim, M.K.; Ahn, S.G.; Kwon, G.S.; Park, Y.H. Optimization of fermentation conditions for production of exopolysaccharide by Bacillus polymyxa. Bioprocess Eng. 1997, 16, 71–75. [Google Scholar] [CrossRef]
  68. Lee, H.K.; Chun, J.; Moon, E.Y.; Ko, S.H.; Lee, D.S.; Lee, H.S.; Bae, K.S. Hahella chejuensis gen. nov., sp. nov., an extracellular-polysaccharide-producing marine bacterium. Int. J. Syst. Evolut. Microbiol. 2001, 51, 661–666. [Google Scholar]
  69. Ramırez-Castillo, M.L.; Uribelarrea, J.L. Improved process for exopolysaccharide production by Klebsiella pneumoniae sp. Pneumoniae by a fed-batch strategy. Biotechnol. Lett. 2004, 26, 1301–1306. [Google Scholar] [CrossRef]
  70. Fialho, A.M.; Moreira, L.M.; Granja, A.; Popescu, A.O.; Hoffmann, K.; Sá-Correia, I. Occurrence, production, and applications of gellan: Current state and perspectives. Appl. Microbiol. Biotechnol. 2008, 79, 889–900. [Google Scholar] [CrossRef]
  71. Marx, J.G.; Carpenter, S.D.; Deming, J.W. Production of cryoprotectant extracellular polysaccharide substances (EPS) by the marine psychrophilic bacterium Colwellia psychrerythraea strain 34H under extreme conditions. Can. J. Microbiol. 2009, 55, 63–72. [Google Scholar] [CrossRef]
  72. Mancuso Nichols, C.; Bowman, J.P.; Guezennec, J. Effects of Incubation Temperature on Growth and Production of Exopolysaccharideby an Antarctic Sea Ice Bacterium Grown in Batch Culture. Appl. Environ. Microbiol. 2005, 71, 3519–3523. [Google Scholar] [CrossRef]
  73. Ko, S.H.; Lee, H.S.; Park, S.H.; Lee, H.K. Optimal conditions for the Production of Exopolysaccharide by Marin Microorganism Hahella chejuensis. Biotechnol. Bioprocess Eng. 2000, 5, 181–185. [Google Scholar] [CrossRef]
  74. Al-Nahas, M.O.; Darwish, M.M.; Ali, A.E.; Amin, M.A. Characterization of an exopolysaccharide-producing marine bacterium, isolate Pseudoalteromonas sp. AM. Afr. J. Microbiol. Res. 2011, 5, 3823–3831. [Google Scholar]
  75. Liu, S.B.; Qiao, L.P.; He, H.L.; Zhang, Q.; Chen, X.L.; Zhou, W.Z.; Zhou, B.C.; Zhang, Y.Z. Optimization of Fermentation Conditions and Rheological Properties of Exopolysaccharide Produced by Deep-Sea Bacterium Zunongwangia profunda SM-A87. PLoS One 2011, 6, e26825. [Google Scholar]
  76. Samain, E.; Milas, M.; Bozzi, L.; Dubreucq, M.; Rinaudo, M. Simultaneous production of two different gel-forming exopolysaccharides by an Alteromonas strain originating from deep-sea hydrothermal vents. Carbohydr. Polym. 1997, 34, 235–241. [Google Scholar] [CrossRef]
  77. Dubreucq, G. Contribution à l’étude Structural d’un Polysaccharide Excrete par la Bacteria Alteromonas sp. 1644 Isolée du Milieu Hydrothermal Profound. Ph.D. Thesis, Université des Sciences et Technologies de Lille, Villeneuve d’Ascq, France, 1996. [Google Scholar]
  78. Rinker, K.D.; Kelly, R.M. Effect of carbon and nitrogen sources on growth dynamics and exopolysaccharide production for the hyperthermophilic archaeon Thermococcus litoralis and bacterium Thermotoga maritima. Biotechnol. Bioeng. 2000, 69, 537–547. [Google Scholar] [CrossRef]
  79. Lapaglia, C.; Hartzell, P.L. Stress-Induced Production of Biofilm in the Hyperthermophile Archaeoglobus fulgidus. Appl. Environ. Microbiol. 1997, 63, 3158–3163. [Google Scholar]
  80. Nicolaus, B.; Lama, L.; Panico, A.; Schiano Moriello, V.; Romano, I.; Gambacorta, A. Production and characterization of exopolysaccharides excreted by thermophilic bacteria from shallow, marine hydrothermal vents of flegrean areas (Italy). Syst. Appl. Microbiol. 2002, 25, 319–325. [Google Scholar] [CrossRef]
  81. More, T.T.; Yan, S.; Hoang, N.V.; Tyagi, R.D.; Surampalli, R.Y. Bacterial polymer production using pre-treated sludge as raw material and its flocculation and dewatering potential. Bioresour. Technol. 2012, 121, 425–431. [Google Scholar]
  82. Razack, A.S.; Velayutham, V.; Thangavelu, V. Medium optimization for the production of exopolysaccharide by Bacillus subtilis using synthetic sources and agro wastes. Turk. J. Biol. 2013, 37, 280–288. [Google Scholar]
  83. Küçükaşik, F.; Kazak, H.; Güney, D.; Finore, I.; Poli, A.; Yenigün, O.; Nicolaus, B.; Toksoy, E.O. Molasses as Fermentation Substrate for Levan production by Halomonas sp. Appl. Microbiol. Biotechnol. 2011, 89, 1729–1740. [Google Scholar]
  84. Han, Y.W.; Watson, M.A. Production of microbial levan from sucrose, sugarcane juice and beet molasses. J. Ind. Microbiol. Biotechnol. 1992, 9, 257–260. [Google Scholar]
  85. Banik, R.M.; Santhiagu, A.; Upadhyay, S.N. Optimization of nutrients for gellan gum production by Sphingomonas paucimobilis ATCC-31461 in molasses based medium using response surface methodology. Bioresour. Technol. 2007, 98, 792–797. [Google Scholar] [CrossRef]
  86. Kalogiannis, S.G.; Iakovidou, M.; Liakopoulou-Kyriakides, D.A.; Skaracis, G.N. Optimization of xanthan gum production by Xantomonas campestris grown in molasses. Process Biochem. 2003, 39, 249–256. [Google Scholar] [CrossRef]
  87. Plackett, R.L.; Burman, J.P. The design of optimum multifactorial experiments. Biometrika 1946, 33, 305–325. [Google Scholar]
  88. Qiang, L.; Yumei, L.; Sheng, H.; Yingzi, L.; Dongxue, S.; Dake, H.; Jiajia, W.; Yanhong, Q.; Yuxia, Z. Optimization of Fermentation Conditions and Properties of an Exopolysaccharide from Klebsiella sp. H-207 and Application in Adsorption of Hexavalent Chromium. PLoS One 2013, 8, e53542. [Google Scholar] [CrossRef]
  89. Jathore, N.R.; Bule, M.V.; Tilay, A.V.; Annapure, U.S. Microbial Levan from Pseudomonas fluorescens: Characterization and Medium Optimization for Enhanced Production. Food Sci. Biotechnol. 2012, 21, 1045–1053. [Google Scholar] [CrossRef]
  90. Qin, Q.L.; Zhang, X.Y.; Wang, X.M.; Liu, G.M.; Chen, X.L.; Xie, B.B.; Dang, H.Y.; Zhou, B.C.; Yu, J.; Zhang, Y.Z. The complete genome of Zunongwangia profunda SM-A87 reveals its adaptation to the deep-sea environment and ecological role in sedimentary organic nitrogen degradation. Genomics 2010, 11. [Google Scholar] [CrossRef]
  91. Qin, Q.L.; Li, Y.; Zhang, Y.J.; Zhou, Z.M.; Zhang, W.X.; Chen, X.L.; Zhang, X.Y.; Zhou, B.C.; Wang, L.; Zhang, Y.Z. Comparative genomics reveals a deep-sea sediment-adapted life style of Pseudoalteromonas sp. SM9913. Int. Soc. Microb. Ecol. J. 2011, 5, 274–284. [Google Scholar]
  92. Hou, S.; Saw, J.H.; Lee, K.S.; Freitas, T.A.; Belisle, C.; Kawarabayasi, Y.; Donachie, S.P.; Pikina, A.; Galperin, M.Y.; Koonin, E.V.; et al. Genome sequence of the deep-sea gamma-proteobacterium Idiomarina loihiensis reveals amino acid fermentation as a source of carbon and energy. Proc. Natl. Acad. Sci. USA 2004, 101, 18036–18041. [Google Scholar] [CrossRef]
  93. Martinez, E.I.; Cuadrado, A.M.; Auria, G.D.; Mira, A.; Ferriera, S.; Johnson, J.; Friedman, R.; Valera, F.R. Comparative genomics of two ecotypes of the marine planktonic copiotroph Alteromonas macleodii suggests alternative lifestyles associated with different kinds of particulate organic matter. Int. Soc. Microb. Ecol. J. 2008, 2, 1194–1212. [Google Scholar]
  94. Rehm, B.H.A., Ed.; Microbial Production of Biopolymers and Polymer Precursors: Applications and Perspectives; Caister Academic Press: Massey, New Zealand, 2009.
  95. Bae, S.O.; Sugano, Y.; Ohi, K.; ShodaBae, M. Features of bacterial cellulose synthesis in a mutant generated by disruption of the diguanylate cyclase 1 gene of Acetobacter xylinum BPR 2001. Appl. Microbiol. Biotechnol. 2004, 65, 315–322. [Google Scholar]
Mar. Drugs EISSN 1660-3397 Published by MDPI AG, Basel, Switzerland RSS E-Mail Table of Contents Alert
Back to Top