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. 2015 Sep 4;31:1823–1844. doi: 10.1007/s11274-015-1937-8

Extracellular polysaccharides from Ascomycota and Basidiomycota: production conditions, biochemical characteristics, and biological properties

Monika Osińska-Jaroszuk 1,✉, Anna Jarosz-Wilkołazka 1, Jolanta Jaroszuk-Ściseł 2, Katarzyna Szałapata 1, Artur Nowak 2, Magdalena Jaszek 1, Ewa Ozimek 2, Małgorzata Majewska 2
PMCID: PMC4621709  PMID: 26340934

Abstract

Fungal polysaccharides (PSs) are the subject of research in many fields of science and industry. Many properties of PSs have already been confirmed and the list of postulated functions continues to grow. Fungal PSs are classified into different groups according to systematic affinity, structure (linear and branched), sugar composition (homo- and heteropolysaccharides), type of bonds between the monomers (β-(1 → 3), β-(1 → 6), and α-(1 → 3)) and their location in the cell (cell wall PSs, exoPSs, and endoPSs). Exopolysaccharides (EPSs) are most frequently studied fungal PSs but their definition, classification, and origin are still not clear and should be explained. Ascomycota and Basidiomycota fungi producing EPS have different ecological positions (saprotrophic and endophytic, pathogenic or symbiotic-mycorrhizae fungi); therefore, EPSs play different biological functions, for example in the protection against environmental stress factors and in interactions with other organisms. EPSs obtained from Ascomycota and Basidiomycota fungal cultures are known for their antioxidant, immunostimulating, antitumor, and antimicrobial properties. The major objective of the presented review article was to provide a detailed description of the state-of-the-art knowledge of the effectiveness of EPS production by filamentous and yeast Ascomycota and Basidiomycota fungi and techniques of derivation of EPSs, their biochemical characteristics, and biological properties allowing comprehensive analysis as well as indication of similarities and differences between these fungal groups. Understanding the role of EPSs in a variety of processes and their application in food or pharmaceutical industries requires improvement of the techniques of their derivation, purification, and characterization. The detailed analyses of data concerning the derivation and application of Ascomycota and Basidiomycota EPSs can facilitate development and trace the direction of application of these EPSs in different branches of industry, agriculture, and medicine.

Keywords: Exopolysaccharides, Fungi, Ascomycota, Basidiomycota, Biological properties

Introduction

Microbiological polysaccharides (PSs) are classified into different groups according to their location in the cell, structure, sugar composition, type of bonds between monomers, and systematic affinity. Exopolysaccharides (EPSs) are the most frequently studied microbial PSs, besides cell wall PSs and intracellular cytosolic PSs. Several definitions of EPS are reported in the literature (Mahapatra and Banerjee 2013b). In many cases, EPSs are rather defined by the separation/extraction method used than by theoretical consideration of the composition of the cell wall and macromolecules outside the cell wall. Bound or soluble EPSs contain not only high-molecular-weight polymeric compound exudates from microorganisms, but also products of cellular lysis and hydrolysis of macromolecules.

EPSs are particularly intensively studied in bacterial cultures, where they are synthesized in high concentrations in young cultures growing on various carbon (C) and nitrogen (N) sources, but at a relatively high temperature (Donot et al. 2012). Filamentous and yeast Ascomycota and Basidiomycota fungi are used for biotechnological derivation of EPSs in laboratory conditions using similar techniques, culture conditions, sources of C, N and other elements, culture periods, and mostly acidic pH of the medium (Shu and Lung 2004; Mahapatra and Banerjee 2013b). Fungal strains belonging to both these groups are an important component, characterized by the highest biomass, of the microbiome of various environments (Olsson et al. 1999). It worth mentioning that the optimal period of EPS synthesis by these fungi does not correspond to the period of biomass formation (Madla et al. 2005; Shih et al. 2008). Ascomycota and Basidiomycota fungi exhibit a very high variation of the weight of synthesized EPSs and their biochemical and biological properties (Donot et al. 2012; Mahapatra and Banerjee 2013b).

Microbial PSs are the subject of research in many fields of science. Many properties of PSs have already been confirmed and the list of postulated functions continues to grow. The directions of research on PSs are mainly focused on identification of factors responsible for their synthesis/release, optimization of production (connected with the cost and productivity), and elucidation of the role and application of PSs in interactions between various organisms. The knowledge of the diversity of fungal PSs and the mode of interaction between PSs with microorganisms and higher organisms is still limited, since identification of PSs and investigation of the mechanisms of this interaction depends on the availability of isolation and diagnostics methods.

PS isolation methods are based on fractionation and use of various solvents and PS procedures. Lack of uniformity in these methods often makes the results of different studies incomparable, or even contradictory. Understanding the role of PSs in a variety of processes and the application of PSs in food or pharmaceutical industries or as plant resistance inducers (elicitors) requires improvement of the techniques of derivation, purification, and exploration of properties. The process of PS derivation involves selection of suitable microorganisms, the type of culture, and the method for PS preparation/extraction. Fungal EPSs are derived through ethanol precipitation with different proportions of the culture/water suspension and alcohol (Shu and Lung 2004; Chen et al. 2011; Ma et al. 2015).

Exploration of the similarities and differences in the conditions as well as the efficiency of EPS production and derivation is of great importance as it could contribute to standardization of technologies and selection of optimum production conditions and techniques of purification of fungal EPSs. Very important is also identification of the similarities and differences in the structure and properties of EPSs produced by Ascomycota and Basidiomycota strains, which could facilitate development of mixed formulas containing both Ascomycota and Basidiomycota mycelia or the EPSs of these strains. Given the complementarity of their components, such preparations should have a broader spectrum of activity in various fields of biotechnology, medicine, agriculture, and environmental protection.

Production of EPS by Ascomycota and Basidiomycota fungal strains

Parameters of the growth medium and culture conditions

Recently, many fungal filamentous and yeast Ascomycota and Basidiomycota strains, are known for their ability to produce EPSs in various culture conditions. The most commonly encountered EPS producers from these both group of microorganisms and parameters of culture growth facilitating EPS production are collected, selected, and presented in Table 1.

Table 1.

Ascomycota and Basidiomycota strains producing EPS: the composition of growth medium and the culture conditions

EPS producer Main parameters of growth medium, type of medium and concentration of components (g l−1) Culture conditions EPS yield (g l−1) References
Carbon source Nitrogen source Salts Type of culture (rev. min−1) Temperature (°C) Initial pH Optimal time (day)
Ascomycota
 Alternaria alternate Glucose (40) YE (20) KH2PO4 (0.5), MgSO4·7H2O (0.5) Shaking (150) 30 6.58 9 11.96 Nehad and El-Shamy (2010)
 Aspergillus sp. Y16 Glucose (20) YE (3), Peptone (5), ME (3) KH2PO4 (0.5), NH4Cl (0.5), Sea salt (24.4) Shaking (–) 25 6.0–6.5 7 0.60 Chen et al. (2011)
 Aspergillus sp. RYLF17 Glucose (–) PE in PDB – Fermentation 30 6.0 14 0.60 Yadava et al. (2012)
 Aspergillus versicolor Sorbitol (20), maltose (20) MG (10), YE (3), tryptophane (0.5) KH2PO4 (0.5), MgSO4·7H2O (0.3), sea salt (33.3) – 20 6.5 30 0.24 Chen et al. (2013a)
 Aureobasidium pullulans RYLF-10 Sucrose (50) YE (1) NaCl (0.1), K2HPO4 (0.1), MgSO4 (0.1) Shaking (–) 28 5.0 7 42.24 Yadav et al. (2014)
 Botryosphaeria rhodina MMLR Sucrose (50) NH4NO3 (2) VMSM* Shaking (180) 28 – 3 1.80 Barbosa et al. (2003) and Vasconcelos et al. (2008)
 Botryosphaeria rhodina MMGR Sucrose (50) NH4NO3 (2) VMSM* Shaking (180) 28 – 3 1.50
 Botryosphaeria rhodina MMMFR Sucrose (50) NH4NO3 (2) VMSM* Shaking (180) 28 – 3 0.40
 Botryosphaeria rhodina MMPI Sucrose (50) NH4NO3 (2) VMSM* Shaking (180) 28 – 3 1.30
 Botryosphaeria rhodina DABAC-P82 Glucose (30) NaNO3 (2), YE (1) KH2PO4 (1), MgSO4·7H2O (0.5), KCl (0.5) Shaking (150) 28 3.7 1 17.70 Selbmann et al. (2003)
 Cordyceps sinensis Cs-HK1 Sucrose (40) YE (10), peptone (5) KH2PO4 (1), MgSO4·7H2O (0.5) Shaking (150) 20 6.8 7 1.02 Leung et al. (2009) and Huang et al. (2013)
 Fusarium coccophilum BCC2415 Glucose (–) PE in PDB – Shaking (150) 25 – 21 2.83 Madla et al. (2005)
 Fusarium oxysporum JN604549 Glucose (20) YE (3), peptone (5), ME (3) KH2PO4 (0.5), NH4Cl (0.5), sea salt (24.4) Fermentation 25 6.0–6.5 40 0.59 Chen et al. (2015)
 Fusarium oxysporum Dzf17 Glucose (50) Peptone (13) KH2PO4 (0.6), MgSO4·7H2O (0.2), NaCl (0.6) Shaking (150) 25 – 14 0.21 Li et al. (2014)
 Fusarium oxysporum Y24-2 Glucose (20) YE (3), peptone (5), NH4Cl (0.5) KH2PO4 (0.5), NH4Cl (0.5) Shaking (–) 25 6.0–6.5 7 0.12 Guo et al. (2010, 2013)
 Fusarium solani SD5 Glucose (9.8), PDB YE (0.69), PE in PDB KH2PO4 (0.5), KCl (0.5) Shaking (120) 28 6.46 13.7 2.28 Mahapatra and Banerjee (2012)
 Hypocreales sp. NCHU01 Sucrose (10.6) YE (10.92) KH2PO4 (1), MgSO4 (1) Shaking (100) 25 6.5 5 1.33 Yeh et al. (2014)
 Morchella crassipes Maltose (44.8) Tryptone (4.21) – Shaking (150) 28 6.0 7 9.67 He et al. (2012)
 Penicillium commune Mannitol (20), Maltose (20), Glucose (10) MG (10), corn syrup (1), YE (3) KH2PO4 (0.5), MgSO4·7H2O (0.3), CaCO3 (20), sea salt (33) Fermentation 28 6.5 10 0.43 Chen et al. (2013c)
 Penicillium griseofulvum Maltose (20), Glucose (10), Mannitol (20) MG (10), YE (3), maize paste (1) KH2PO4 (0.5), MgSO4 (0.3) Static 20 6.5 30 0.25 Chen et al. (2013b)
 Penicillium vermiculatum CCM F-276 Glucose (90) NaNO3 (2) KH2PO4 (1), KCl (0.5), MgSO4·7H2O (0.5), FeSO4·7H2O (0.01), CuSO4·5 H2O (0.025) Shaking (–) 28 6.3 7 4.8 Kogan et al. (2002)
 Phoma herbarum CCFEE 5080 Sorbitol (60) NaNO3 (3) KCl (0.5), KH2PO4 (1), MgSO4·7H2O (0.5) Shaking (150) 28 4.7 4 13.6 Selbmann et al. (2002)
 Trichoderma pseudokoningii Glucose (–) PE (–) – Shaking (180) 28 – 10 – Huanga et al. (2012)
Basidiomycota
 Agaricus nevoi HAI 610 Mannitol (20) Corn steep liquor (20 mM), YE (3) KH2PO4 (0.8), Na2HPO4 (0.4), MgSO4·7 H2O (0.5) Shaking (150) 25 6.0 5 3.00 Elisashvili et al. (2009)
 Antrodia camphorate Glucose (25) Peptone (5), ME (3), YE (3) KH2PO4·1 H2O (1), MgSO4·7 H2O (1) Batch fermentation (300) 28 5.0 14 0.12 Shu and Lung (2004)
 Antrodia cinnamomea BCRC 35396 Glucose (50) ME (3), YE (3), calcium nitrate (5) KH2PO4·1 H2O (1), MgSO4·7 H2O (1) Shaking (150) 28 5.5 14 0.58 Lin and Sung (2006)
 Auricularia auricula AA-2 Glucose (40) Soybean powder (7) KH2PO4 (4), MgSO4·7 H2O (2) Batch fermentation (200) 28 5.4 4 7.50 Wu et al. (2006)
 Clavariadelphus truncates PDB (24) ME (10), peptone (1) – Shaking (150) 25 – 7 – Demir and Yamaç (2008)
 Cerrena unicolor PDB (24) ME (10), peptone (1) – Shaking (150) 25 – 7 – Demir and Yamaç (2008)
 Cerrena maxima IBB 681 Maltose (20) YE (3), (NH4)2SO4 (2) KH2PO4 (0.8), Na2HPO4 (0.4), MgSO4·7 H2O (0.5) Shaking (150) 25 6.0 5 1.20 Elisashvili et al. (2009)
 Coprinus comatus PDB (24) ME (10), peptone (1) – Shaking (150) 25 – 7 – Demir and Yamaç (2008)
 Cryptococcus laurentii DSMZ 70766 Sucrose (35) YE (3) Na2HPO4·12 H2O (2.5), MgSO4·7 H2O (0.5) Fermentation (150) 25 6.0 6 4.3 Smirnou et al. (2014)
 Cryptococcus neoformans ATCC 24067 Glucose (2.7) Glycine (1), thiamine (0.001) MgSO4 (1.2), KH2PO4 (4) – 30 5.5 – – Frases et al. (2008)
 Flammulina velutipes SF-06 Glucose (10) Potato (cut into pieces) (200) KH2PO4 (1.5), MgSO4·7 H2O (1) Batch fermentation 25 – 7 – Ma et al. (2015)
 Fomes fomentarius Glucose (60) Silkworm chrysalis (15), YE (3) KH2PO4 (1), MgSO4·7 H2O (0.8), CaCl2 (0.5) Shaking (150) 25 6.0 8 3.64 Chen et al. (2008a, b)
 Ganoderma applanatum KFRI 646 Glucose or maltose (60) YE (2), glutamic acid (1) KH2PO4 (2), MgSO4 (0.5) Shaking (100) 25 4.5 12 1.35 Lee et al. (2007)
 Ganoderma carnosum PDB (24) ME (10), peptone (1) – Shaking (150) 25 – 7 – Demir and Yamaç (2008)
 Ganoderma lucidium UF20706 Glucose (17.5) Peptone (2.5), wheat grains, extract (–) KH2PO4 (1.5), MgSO4·7 H2O (1) Shaking (150) 25 4.0 14 0.53 Fraga et al. (2014)
 Ganoderma lucidum CCGMC 5.616 Lactose (35) YE (5), Peptone (5) KH2PO4 (1), MgSO4·7 H2O (0.5) Fed-batch fermentation (–) 30 – 14 1.25 Tang and Zhang (2002)
 Ganoderma lucidium HAI 447 Glucose (20) YE (3), (NH4)2SO4 (2) KH2PO4 (0.8), Na2HPO4 (0.4), MgSO4·7 H2O (0.5) Shaking culture (150) 25 6.0 5 1.6 Elisashvili et al. (2009)
 Grifola frondosa Glucose (40) YE (8) Corn steep powder (12) (NH4)2SO4 (1) MSS** Fed-batch fermentation (250) 25 5.0 13 3.88 Shih et al. (2008)
 Inonotus levis HAI 796 Glucose (20) Corn steep liquor (20 mM) YE (3) KH2PO4 (0.8), Na2HPO4 (0.4), MgSO4·7 H2O (0.5) Shaking (150) 25 6.0 5 3.00 Elisashvili et al. (2009)
 Laetiporus sulphureus PDB (24) ME (10), peptone (1) – Shaking (150) 25 – 7 – Demir and Yamaç (2008)
 Lentinus edodes Beer wort (7° of Balling’s scale) – – Batch fermentation (150) 25 – 4 4.00 Lobanok et al. (2003)
 Lentinus strigosus PDB (24) ME (10), peptone (1) – Shaking (150) 25 – 7 – Demir and Yamaç (2008)
 Lenzites betulina PDB (24) ME (10), peptone (1) – Shaking (150) 25 – 7 –
 Phellinus gilvus Glucose (30) Corn steep powder (5) KH2PO4 (0.68), K2HPO4 (0.87), MgSO4·7 H2O (1.23) Batch fermentation 30 4.0 11 5.30 Hwang et al. (2003)
 Phellinus igniarius HAI 795 Maltose (20) YE (3), (NH4)2SO4 (2) KH2PO4 (0.8), Na2HPO4 (0.4), MgSO4·7 H2O (0.5) Shaking (150) 25 6.0 5 1.80 Elisashvili et al. (2009)
 Phellinus sp. P0988 Glucose (50) Glutamic acid (4), (NH4)2SO4 (4) KH2PO4 (1), MgSO4 (1) Batch fermentation (–) 28 6.5 5 10.90 Ma et al. (2014)
 Pleurotus dryinus IBB 903 Glucose (20) YE (3), (NH4)2SO4 (2) KH2PO4 (0.8), Na2HPO4 (0.4), MgSO4·7 H2O (0.5) Shaking (150) 25 6.0 5 1.10 Elisashvili et al. (2009)
 Pleurotus pulmonarius Galactose (30) YE (4) KH2PO4 (1), MgSO4·7 H2O (0.2) Shaking (120) 22 – 18 0.42 Smiderle et al. (2012)
 Pleurotus sajor-caju CCB 019 Glucose (20) (NH4)2SO4 (5), YE (2), Peptone (1) KH2PO4 (1), MgSO4·7 H2O (0.2) Shaking (120) 30 6.5-7.0 – – Telles et al. (2011)
 Pleurotus sajor-caju Glucose (20) (NH4)2SO4 (2.5), peptone (1) KH2PO4 (1), MgSO4·7 H2O (0.2), CaCO3 (1) Batch fermentation (300) 30 4.0 20 0.94 Silveira et al. (2015)
 Polyporus arcularius PDB (24) ME (10), peptone (1) – Shaking (150) 25 – 7 – Demir and Yamaç (2008)
 Trametes versicolor Fructose (20) YE (2), peptone (1), (NH4)2SO4 (5) KH2PO4 (1), MgSO4·7 H2O (0.2) Shaking (–) 27 6.0 7 8.00 Bolla et al. (2010)
 Trametes versicolor IBB 897 Maltose (20) YE (3), (NH4)2SO4 (2) KH2PO4 (0.8), Na2HPO4 (0.4), MgSO4·7 H2O (0.5) Shaking (150) 25 6.0 5 1.40 Elisashvili et al. (2009)
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ME malt extract, MG monosodium glutamate, YE yeast extract, PDB potato dextrose broth, PE potato extract, VMSM vogel minimum salt medium, MSS mineral salt solution

VMSM* composition: Na3 citrate—2.5 g l−1, KH2PO4—5.0 g l−1, NH4NO3—2.0 g l−1, MgSO4·7H2O—0.2 g l-1, CaCl2·2H2O—0.1 g l−1, biotin—25 mg l−1, citric acid—5.0 mg l−1, ZnSO4·7H2O—5.0 mg l−1, Fe(NH4)2(SO4)2·6H2O—1.0 mg l−1, CuSO4·5H2O—0.25 mg l−1, MnSO4·H2O—0.05 mg l−1, H3BO3—0.05 mg l−1, NaMoO4·2H2O—0.05 mg l−1; MSS* composition: MgSO4·7H2O—1.20 g l−1, NaCl—0.06 g l−1, KH2PO4—0.20 g l−1, CaCl2—0.20 g l−1, FeSO4·7H2O—0.10 g l−1, ZnCl2—0.018 g l−1

The growth conditions of the fungus e.g. the type of culture, temperature, pH value, C and N source, appropriate salt content, and time of culture are essential for the type and amount of EPS obtained. The maximal yield of EPS produced by Ascomycota and Basidiomycota fungi was in the range from 0.12 to 42.24 g l−1 and depended mainly on the tested strain and culture conditions used (Table 1). The production of fungal EPS was reached in shaking cultures with a constant supply of oxygen. Bolla et al. (2010) examined production of EPS by Trametes versicolor and reported that the yield of EPS in shaking cultures was 8.0 g l−1. In turn, also the batch fermentation technique for EPS production (10.92 g l−1) by Phellinus sp. PO988 was very effective among Basidiomycota strains (Ma et al. 2014). The greatest efficiency in EPS production, i.e. up 42.24 g l−1, was reported by Yadav et al. (2014) in cultures of the Ascomycota fungus Aureobasidium pullulans RYLF-10. The cultivation time is also an important factor affecting EPS production and depends mainly on the type of culture and the type of the fungal strain. The optimal time for EPS synthesis in cultures of Ascomycota and Basidiomycota strains usually ranges from 3 to 40 days (Table 1). It is known that the most effective EPS synthesis occurs at the end of the logarithmic growth phase or early stationary phase. In contrast to bacteria, Ascomycota and Basidiomycota fungi usually require a long incubation time to produce more EPS although Wu et al. (2006) showed that Auricularia auricula produced relatively large amounts of EPS (7.5 g l−1) after 4 days of growth and Ascomycota Botryosphaeria rhodina strain DABAC-P82 synthesized up to 17.7 g l−1 of EPS after only 1 day of culture (Selbmann et al. 2003). An excessively long cultivation time contributed to reduction of EPS amounts in the liquid medium and was related to formation of low molecular EPS (Shu and Lung 2004). For example, Chen et al. (2015) obtained only 0.59 g l−1 of EPS after 40 days of Fusarium oxysporum JN604549 cultivation. Ascomycota and Basidiomycota strains produced amounts of maximum EPS at a temperature range between 20 and 30 °C. In turn, the pH values of the culture medium are usually acidic or neutral and oscillate around a range of 4.0–7.0 for maximum EPS production. It was observed that the pH values varied during the cultivation days. For example, B. rhodina DABAC-P82 strains changed the initially acidic pH value from 3.7 to 5.9–6.5 after 1 day of cultivation (Selbmann et al. 2003). The EPS production efficiency depends on the type of the C source. The main source of C in most Ascomycota and Basidiomycota cultures was glucose, but potato dextrose broth (PDB) and sugars such as sucrose, maltose, mannitol, lactose, and fructose were used as well. The concentration of the compound serving as a C source is an additional important factor in the synthesis of EPSs. It has been shown that the most optimal concentration of the C source usually varies between 30 and 50 g l−1 (Table 1). Another important factor in the production of EPS in fungi is the presence of organic N sources (e.g. corn steep liquor, yeast extract, peptone, malt extract, soybean powder) and inorganic N sources comprising ammonium sulfate, sodium nitrate, and ammonium chloride, as well as mineral salts in the growth medium (Table 1). The highest yield (10.9 g l−1) of Basidiomycota EPS was obtained in the Phellinus sp. P0988 culture with glutamic acid and ammonium sulfate (4 g l−1) used as the main N sources and glucose (50 g l−1) as the main C source (Ma et al. 2014). The highest yield (42.2 g l−1) of Ascomycota EPS was described for Aureobasidium pullulans culture with yeast extract (1 g l−1) and sucrose (50 g l−1) as the main N and C sources, respectively (Yadav et al. 2014).

In cultures of Ascomycota B.rhodina strain, a Vogel Minimum Salt Medium (VMSM) with ammonium nitrate as the main N source but also with biotin and traces (1.0 mg l−1) of ammonium ferrous sulfate was used (Barbosa et al. 2003; Vasconcelos et al. 2008). This VMSM and mineral salt solution (MSS) used in Basidiomycota Grifola frondosa strain culture was a very rich source of different salts (Table 1). Phosphorous and magnesium are components of almost all cultures used for derivation of fungal EPSs and seem a most important mineral additives stimulating EPS production. Such compounds as potassium dihydrogen phosphate (KH2PO4) and dipotassium hydrogen phosphate (K2HPO4) are most effectively used by fungi as a phosphorus source. In addition, magnesium sulfate (MgSO4·7H2O), sodium phosphate (Na2HPO4), sodium chloride, and potassium chloride are usually used for supplementation of media for cultivation of EPS producers.

EPSs isolation, extraction, and purification methods

In contrast to cell-wall or cytosolic PSs, EPSs do not require drastic methods of extraction with hot water or organic solvents (Madla et al. 2005; Chen et al. 2008a, b; Mahapatra and Banerjee 2013a). Usually, to obtain crude EPS, the culture fluid is precipitated by alcohols such as ethanol (absolute or 95 %) or methanol and only in some cases by acetone or isopropanol at a temperature of 4 °C for a period of 12–24 h (Table 2). The main extraction method of EPS obtaining from Ascomycota and Basidiomycota strains cultures is the precipitation with 95 % ethanol used in a proportion 1/4 (v/v) of supernatant and ethanol. Particularly in Ascomycota strains, primary purification of supernatant with 5 % trichloroacetic acid (TCA) is sometimes applied (Yadava et al. 2012). After dialysis against water, crude EPSs are generally stored as vacuum-dried or lyophilized powder. The next step of EPS purification is deproteinization thereof using Sevage reagent (Chen et al. 2011, 2013a, b, c). The main methods used for purification of Ascomycota and Basidiomycota EPSs are Ion Exchange Chromatography (IEC) and a type of Size Exclusion Chromatography (SEC)–Gel Permeation Chromatography (GPC) (Table 2) (Shu and Lung 2004; Chen et al. 2011; Ma et al. 2015).

Table 2.

EPS of Ascomycota and Basidiomycota strains—isolation, extraction, and purification methods

EPS producer The main steps during the procedure of EPS characteristics References
Isolation Purification Solubility Compositions Linkage type Mw (kDa)
Precipitation method (supernatants/alcohol proportion v/v) Period of dialysis against water (h) EPS solution Chromatographic methods
Ascomycota
 Alternaria alternate 95 % ethanol (1/5), 16 h, 4 °C – – – – – – – Nehad and El-Shamy (2010)
 Aspergillus sp. Y16 95 % ethanol (1/3) 48 Water IEC
GPC		 Water EPS1-Man, Gal
EPS2-Man, Glc		 EPS1—1 → 2;1 → 6,
EPS2—1 → 3; 1 → 6		 EPS1-15.0
EPS2-6.0		 Chen et al. (2011)
 Aspergillus sp. RYLF17 95 % ethanol (1/4), 24 h, 4 °C – – – – – – – Yadava et al. (2012)
 Aspergillus versicolor 95 % ethanol (1/3) 48 Water IEC
GPC		 Water Glc, Man α-1 → 6 500.0 Chen et al. (2013a)
 Aureobasidium pullulans RYLF-10 95 % ethanol (1/4), 24 h, 4 °C – Water – – – – – Yadav et al. (2014)
 Botryosphaeria rhodina MMLR Absolute ethanol (1/3) 48 GPC Water, 1 M NaOH Glc β-1 → 6 – Barbosa et al. (2003) and Vasconcelos et al. (2008)
 Botryosphaeria rhodina MMGR Absolute ethanol (1/3) 48 GPC Water, 1 M NaOH Glc β-1 → 6 –
 Botryosphaeria rhodina MMPI Absolute ethanol (1/3) 48 GPC Water, 1 M NaOH Glc β-1 → 6 –
 Botryosphaeria rhodina MMMFR Absolute ethanol (1/3) 48 Water GPC Water, 1 M NaOH Glc β-1 → 3
β-1 → 6		 –
 Botryosphaeria rhodina DABAC-P82 Ethanol (1/2), 16 h, 4 °C, repeated twice 24 Water GPC Water Glc β-1 → 6
β-1 → 3		 4.9 Selbmann et al. (2003)
 Cordyceps sinensis Cs-HK1 95 % ethanol (5 ratios: 1/0.2, 1/0.4, 1/1, 1/2, 1/5) – – – – Glc – EPS0.2-47,400.0
EPS0.4-47,400.0
EPS1-253,000.0
EPS2-630.0
EPS5-16.0		 Leung et al. (2009) and Huang et al. (2013)
 Fusarium coccophilum BCC2415 95 % ethanol (1/4), 12 h, −20 °C – Water GPC Water – – 2.8 Madla et al. (2005)
 Fusarium oxysporum JN604549 95 % ethanol (1/3) 72 Water IEC
GPC		 Water Gal, Glc, Man β-1 → 6
β-1 → 2		 61.2 Chen et al. (2015)
 Fusarium oxysporum Dzf17 95 % ethanol (1/3), 48 h, 4 °C – Water – Water – – – Li et al. (2014)
 Fusarium oxysporum Y24-2 95 % ethanol (1/4) 72 Water IEC
GPC		 Water Gal, Glc α-1 → 2
β-1 → 6		 36.0 Guo et al. (2010, 2013)
 Fusarium solani SD5 Absolute ethanol (1/5), 24 h, 4 °C 24 Water GPC Water Gal, Rha α-1 → 2
β-1 → 4
α-1 → 6		 187.0 Mahapatra and Banerjee (2012)
 Hypocreales sp. NCHU01 95 % ethanol (1/4) – – – 1 M NaOH 60 °C, 1 h – – – Yeh et al. (2014)
 Morchella crassipes 95 % ethanol (1/4), 16 h, 4 °C – 0.2 M NaCl GPC 0.2 M NaCl – – 19.6 He et al. (2012)
 Penicillium commune 95 % ethanol (1/3) 48 Water IEC
GPC		 Water Glc, Man, Gal α-1 → 2
β-1 → 6		 18.3 Chen et al. (2013c)
 Penicillium griseofulvum 95 % ethanol (1/3) 48 Water IEC
GPC		 Water Man, Gal α-1 → 2
β-1 → 5
α-1 → 6		 20.0 Chen et al. (2013b)
 Penicillium vermiculatum CCM F-276 Ethanol (1/4) repeated three times – Water GPC Water Glc, Gal, Man β-1 → 6
β-1 → 3		 77.0 Kogan et al. (2002)
 Phoma herbarum CCFEE5080 Absolute ethanol (1/2), 16 h, 4 °C, repeated twice 24 Water GPC Water Glc β-1 → 3
α-1 → 6		 7.4 Selbmann et al. (2002)
 Trichoderma pseudokoningii 95 % ethanol (1/3), 16 h, 4 °C – Water IEC
GPC		 Water Rha, Xyl, Fuc, Man, Glc, Gal – 31.9 Huanga et al. (2012)
Basidiomycota
 Agaricus nevoi HAI 610 95 % ethanol (1/3), 12 h, 20 °C – – – – – – – Elisashvili et al. (2009)
 Antrodia camphorata – 48 Water GPC Water – – EPS1 < 50
EPS2 > 50 < 400
EPS3 > 400		 Shu and Lung (2004)
 Antrodia cinnamomea BCRC 35396 95 % ethanol (1/4), 12 h, 4 °C, repeated twice – – – – – – – Lin and Sung (2006)
 Auricularia auricula AA-2 95 % ethanol, 12 h, 4 °C, repeated twice – – – – – – – Wu et al. (2006)
 Clavariadelphus truncates 95 % ethanol (1/4), 12 h, 4 °C – – – – – – – Demir and Yamaç (2008)
 Cerrena unicolor 95 % ethanol (1/4), 12 h, 4 °C – – – – – – – Demir and Yamaç (2008)
 Cerrena maxima IBB 681 95 % ethanol (1/3), 12 h, 20 °C – – – – – – – Elisashvili et al. (2009)
 Corpinus comatus 95 % ethanol (1/4), 12 h, 4 °C – – – – – – – Demir and Yamaç (2008)
 Cryptococcus laurentii DSMZ 70766 Absolute isopropanol (1/3) – – – – Man, GlcA, Glc, Gal, Xyl – 2000.0 Smirnou et al. (2014)
 Cryptococcus neoformans ATCC 24067 95 % ethanol (1/3), CTAB-PS 24 Water – Water Xyl, GlcA, Man, Gal, Glc – 1210.0 Frases et al. (2008)
 Flammulina velutipes SF-06 95 % ethanol (1/3), 24 h, 4 °C 10 Water ICE
GPC		 – EPS1-Rha, Glc
EPS2-Rha, Gal		 – – Ma et al. (2015)
 Fomes fomentarius 95 % ethanol (1/4), 12 h, 4 °C – – – – – – – Chen et al. (2008a, b)
 Ganderma applanatum KFRI 646 95 % ethanol (1/4), 12 h, 4 °C 72 – – Water Glc, Gal, Man, Xyl – EPS1-2300.0 EPS2-1038.0 Lee et al. (2007)
 Ganoderma carnosum 95 % ethanol (1/4), 12 h, 4 °C – – – – – – – Demir and Yamaç (2008)
 Ganoderma lucidium UF20706 95 % ethanol (1/4), 12 h, 4 °C – – HPAEC – Fuc, Gal, Glc, Man 1 → 3; 1 → 4 – Fraga et al. (2014)
 Ganoderma lucidum CCGMC 5.616 95 % ethanol (–), 12 h, 4 °C – – – Water, NaOH (60 °C) – – – Tang and Zhang (2002)
 Ganoderma lucidium HAI 447 95 % ethanol (1/3), 12 h, 20 °C – – – – – – – Elisashvili et al. (2009)
 Grifola frondosa 95 % ethanol (1/4), 12 h, 4 °C – – GPC 1 M NaOH (60 °C) – – EPS1-390,840.0
EPS2-3097.0		 Shih et al. (2008)
 Inonotus levis HAI 796 95 % ethanol (1/3), 12 h, 20 °C – – – – – – – Elisashvili et al. (2009)
 Laetiporus sulphurous 95 % ethanol (1/4), 12 h, 4 °C – – – – – – – Demir and Yamaç (2008)
 Lentinus edodes 95 % ethanol (1/1), 12 h, 4 °C – – – Water (poor soluble) 0.5 % NaOH – – – Lobanok et al. (2003)
 Lentinus strigosus 95 % ethanol (1/4), 12 h, 4 °C – – – – – – – Demir and Yamaç (2008)
 Lenzites betulina 95 % ethanol (1/4), 12 h, 4 °C – – – – – – –
 Phellinus gilvus 95 % ethanol (1/4), 12 h, 4 °C – Buffer, pH 6.8 SEC/MALS Water Mal, Arab, Xyl, Man, Gal, Glc – EPS1–8 628.0
EPS2–1 045.0
EPS3–610.9 EPS4–335.5		 Hwang et al. (2003)
 Phellinus igniarius HAI 795 95 % ethanol (1/3), 12 h, 20 °C – – – – – – – Elisashvili et al. (2009)
 Phellinus sp. P0988 95 % ethanol (1/3), 12 h, 4 °C – 2 % tannic acid – Water – – – Ma et al. (2014)
 Pleurotus dryinus IBB 903 95 % ethanol (1/3), 12 h, 20 °C – – – – – – – Elisashvili et al. (2009)
 Pleurotus pulmonarius 95 % ethanol (1/3) + – IEC – Man, Gal, Glc
3-O-methyl-Gal		 1 → 3; 1 → 6 – Smiderle et al. (2012)
 Pleurotus sajor-caju CCB 019 Acetone (1/3), 24 h, 4 °C – – – – Man, Gal, Glc
3-O-methyl-Gal		 – – Telles et al. (2011)
 Pleurotus sajor-caju 95 % ethanol – HPAEC – Man, Gal
3-O-methyl-Gal		 1 → 6 64.0 Silveira et al. (2015)
 Polyporus arcularius 95 % ethanol (1/4), 12 h, 4 °C – – – – – – – Demir and Yamaç (2008)
 Trametes versicolor Isopropanol (1/1), 24 h, 4 °C – – – – – – – Bolla et al. (2010)
 Trametes versicolor IBB 897 Absolute ethanol (1/3), 12 h – – – – – – – Elisashvili et al. (2009)
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Arab, arabinose; Fuc, fucose; Gal, galactose; Glc, glucose; GlcA, glucuronic acid; Mal, maltose; Man, mannose; Rha, rhamnose; Xyl, xylose; GPC, Gel Permeation Chromatography type of Size Exclusion Chromatography (SEC); HPAEC, High Performance Anion Exchange Chromatography; IEC, Ion Exchange Chromatography; SEC/MALS, the combination of SEC with Multi-Angle Light Scattering Analysis (MALS); CTAB-PS, isolation of EPS by cetyltrimethylammonium bromide precipitation

EPS characteristics

Ascomycota and Basidiomycota EPSs are usually soluble in water or in a NaCl solution but data concerning the degree of EPS solubility in water are limited. In some cases, solubility of EPSs in alkali solutions (mainly 1 M NaOH) was determined (Table 2). The chemical structures and properties of EPS such as the monosaccharide composition, the linkage type, the molecular weight, or the conformation chain were usually evaluated by different experimental analyses including chromatography technology such as TLC, HPLC, and GLC as well as spectrum analysis such as FTIR and 1D and 2D NMR spectroscopy or GLC-MS (Kozarski et al. 2012; Osińska-Jaroszuk et al. 2014; Silveira et al. 2015). Ascomycota and Basidiomycota EPSs are mainly heteropolysaccharides but in the case of homopolysaccharides glucose is their only monomer (Table 2). The sugar content of various EPSs is varied but glucose, mannose, galactose, xylose, fucose, and rhamnose monomers have frequently been found in fungal EPSs. Moreover, individual monosaccharides synthesized by different groups of Ascomycota and Basidiomycota fungi had different molecular weight (Table 2). EPSs isolated from the Ascomycota and Basidiomycota strains have a different linkage pattern but a 1 → 6 linkage type is dominant, and presence of different types of linkage has been described for Ascomycota EPSs. Guo et al. (2013) reported that EPS from Fusarium oxysporum Y24-2 consists of a disaccharide repeating units with the following structure (n ≈ 111): [→2)-β-d-Galf(1 → 6)-α-d-Glcp(1→](n). A homogenous EPS from Aspergillus versicolor is mainly composed of (1 → 6)-linked α-d-glucopyranose residues, slightly branched by single α-d-mannopyranose units attached to the main chain at C-3 positions of the glucan backbone (Chen et al. 2013a). B. rhodina MMGR produces EPS containing β-1 → 6 branched glucose residues (Barbosa et al. 2003; Vasconcelos et al. 2008). Penicillium griseofulvum produces an EPS composed of a long chain of galactofuranan and a mannose core. The galactofuranan chain consists of (1 → 5)-linked β-galactofuranose, with additional branches at C-6 consisting of (1→)-linked β-galactofuranose residues and phosphate esters. The mannan core is composed of (1 → 6)-linked α-mannopyranose substituted at C-2 by (1→)-linked α-mannopyranose residues, disaccharide, and trisaccharide units of (1 → 2)-linked α-mannopyranose (Chen et al. 2013b). There are only few studies on the linkage type of EPS isolated from Basidiomycota. Silveira et al. (2015) reported that the EPS produced by edible mushrooms Pleurotus sajor-caju was a mannogalactan composed of mannose (37.0 %), galactose (39.7 %), and 3-O-methyl-galactose (23.3 %) and comprised a main chain of (1 → 6)-linked α-d-Galp and 3-O-methyl-α-d-Galp units. Ganoderma lucidium produces EPSs that are mainly β-(1 → 4)-linked branched glucans containing (1 → 3) linkages as well (Fraga et al. 2014).

Bioactive properties and potential biotechnological (medical, environmental, and agricultural) applications of EPS

Many bioactive properties of Ascomycota and Basidiomycota EPSs such as antioxidative, antimicrobial, immunomodulatory, antitumor, hypolipidemic, hypoglycemic, and hepatoprotective activity can find medical applications. The activities of fungal EPSs in such processes as mineral solubilization, heavy metal sorption and hydrocarbon removal as well as eliciting plant resistance created a possibility of potential environmental and agricultural applications of these EPSs in biofertilization, soil/water bioremediation, and plant bioprotection (Table 3). The bioactive properties of PSs are known to depend on many factors, including the structure, monosaccharide components, molecular mass, conformation, configuration of glycosidic bonds, and extraction and isolation methods (Zhou and Chen 2011).

Table 3.

Examples of bioactive properties and potential medical, environmental, and agricultural applications of EPSs obtained from selected Ascomycota and Basidiomycota strains

Bioactivities Ascomycota Basidiomycota
EPS producer References EPS producer References
Potential medical applications
Antioxidative Aspergillus sp. Y16 Chen et al. (2011) Agaricus brasiliensis Kozarski et al. (2011)
Cordyceps sinensis Leung et al. (2009) Ganoderma applanatum Kozarski et al. (2012)
Fusarium oxysporum Chen et al. (2015) Ganoderma lucidium Jia et al. (2009), Liu et al. (2010) and Kozarski et al. (2012)
Morchella crassipes He et al. (2012) Lentinus edodes Kozarski et al. (2012)
Trametes versicolor Kozarski et al. (2012)
Phellinus sp. P0988 Ma et al. (2014)
Flammulina velutipes SF-06 Ma et al. (2015)
Antimicrobial Hirsutella sp. Li et al. (2010) Cerrena unicolor Demir and Yamaç (2008)
Ganoderma applanatum Osińska-Jaroszuk et al. (2014)
Ganoderma carnosum Demir and Yamaç (2008)
Lenzites betulina Demir and Yamaç (2008)
Polyporus arcularius Demir and Yamaç (2008)
Immunomodulatory Fusarium coccophilum BCC2415 Madla et al. (2005) Ganoderma applanatum Osińska-Jaroszuk et al. (2014)
Cordyceps sinensis Zhang et al. (2010) Pleurotus sajor-caju Silveira et al. (2015)
Cryptococcus neoformans Frases et al. (2008)
Antitumor Trichoderma pseudokoningii Huanga et al. (2012) Agaricus blazei Yu et al. (2009)
Cordyceps militaris Kim et al. (2010) Fomes fomentarius Chen et al. (2008a, b)
Cordyceps sinensis Zhang et al. (2010) Ganoderma applanatum Osińska-Jaroszuk et al. (2014)
Ganoderma tsugae Hsu et al. (2008)
Pleurotus sajor-caju CCB 019 Telles et al. (2011)
Wound management Cryptococcus laurentii Smirnou et al. (2014)
Hypoglycemic Cordyceps militaris Kim et al. (2001) Tremella fuciformis Cho et al. (2007)
Lentinus edodes Yang et al. (2002) Phellinus baumii Cho et al. (2007)
Botryosphaeria rhodina Miranda-Nantes et al. (2011) Lentinus edodes Kim et al. (2001)
Phellinus linteus Kim et al. (2001)
Cerrena unicolor Kim et al. (2001)
Coprinus comatus Yamac et al. (2009)
Lenzites betulina Yamac et al. (2009)
Hypolipidemic Cordyceps militaris Yang et al. (2000) Lentinus edodes Kim et al. (2001)
Botryosphaeria rhodina Miranda-Nantes et al. (2011) Phellinus linteus Kim et al. (2001)
Hepatoprotective Antrodia cinnamomea Ho et al. (2008)
Potential environmental and agricultural application
Mineral solubilization (biofertilization) Penicillium sp. Wakelin et al. ( 2004) Pleurotus ostreatus Seneviratne et al. (2008)
Heavy metal sorption (bioremediation) Aspergillus fumigatus Lian et al. (2008)
Hansenula anomala CCY 38-1-22 Breierová et al. (2002)
Colletotrichum sp. Da Silva et al. (2014)
Pestalotiopsis sp. KCTC 8637 Moon et al. (2006)
Aureobasidium pullulans CH1 Radulović et al. (2008)
Hydrocarbon removal (bioremediation) Flavodon flavus NIOCC#312 Raghukumar et al. (2006)
Eliciting plant resistance (bioprotection) Fusarium oxysporum Dzf17 Li et al. (2011)
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Potential medical applications

Given their diversity, fungal EPSs could be used in medicine, for example as antioxidant and antimicrobial agents applied for acceleration of wound healing and fighting bacterial and viral infections as well as antitumor agents activating immune response in the host and supporting chemotherapy treatment (Zhang et al. 2002, 2007; Chen and Seviour 2007; Liu et al. 2009).

Antioxidative and antimicrobial activities

Antioxidative properties have been described for fungal compounds, mainly represented by phenolic compounds, β-tocopherol and β-carotene, PS-protein complexes, and EPSs (Palacios et al. 2011). Until now, it has been demonstrated that ethanol extracts of nearly 150 species of fungi exhibit antioxidative activity (Chang and Miles 2004). These antioxidative properties have been recognized for several EPSs of both Ascomycota and Basidiomycota strains (Table 3). Antioxidant activity assigned to PSs consists in chelation of ferrous ions Fe2+ or prevention of Fenton’s reaction and inhibition of lipid peroxidation as well as enhancement of the enzymatic activity of the antioxidant system such as superoxide dismutase, catalase, or glutathione peroxidase (Kozarski et al. 2014). Antioxidants may react directly with reactive oxygen species or indirectly by reduced oxidation reaction metabolites, not allowing formation of oxygen free radicals. Therefore, PSs show greater antioxidant properties than monosaccharides because the most important factor that has an influence on the ability of EPSs to scavenge free radicals is the size of the carbohydrate molecule. The choice of a proper method of extraction of PS and PS–protein complexes, especially the type of applied solvents, also affects the antioxidant activity of purified preparations. For example, water extracts of fungal PSs contain proteins and phenol compounds with antioxidant activity (Zhou and Chen 2011; Kozarski et al. 2014).

There are many reports available describing the antibacterial properties of fungal EPSs, especially those from Basidiomycota strains from the genus Cerrena, Ganoderma, Lenzites and Polyporus, in relation to both gram-positive and gram-negative bacteria (Demir and Yamaç 2008). EPS from Ganoderma applanatum showed antibacterial properties against Staphyloccoccus aureus and a toxic effect against Vibrio fischeri cells (Osińska-Jaroszuk et al. 2014). For Ascomycota (Hirsutella strain) EPS, also antimicrobial activity against Bacillus subtilis and Micrococcus tetragenus was studied (Li et al. 2010).

Immunomodulatory and antitumor activities and wound management

Antitumor activity of PSs is closely related to their immunomodulatory and immunostimulant activity, which is affected by many physical and chemical properties. Particles of β-(1 → 3) glucans with the molecular weight less than 20 kDa have either no or low immunomodulatory activity (Bohn and BeMiller 1995). There is a correlation between the conformation and weight of the molecule because only a molecule with molecular weight of at least 90 kDa may take a triple helix structure. There are a number of papers on the immunomodulatory and antitumor action of EPSs from both Ascomycota and Basidiomycota strains (Table 3). Lee et al. (2007) has demonstrated that the effect of EPS from G. applanatum on TNF-α was dependent on its molecular size. Within the range of fungal PS, the most active antitumor properties are exhibited by β-glucans binding by β-(1 → 3)-glycosidic bonds. Not without significance is also the additional share of side chains linked by β-(1 → 6) glycosidic bonds affecting the degree of branching molecules, which is reflected in increased antitumor activity of β-(1 → 3) glucan (Chen and Seviour 2007). The action of PS mainly involves stimulation of macrophages and dendritic cells (Kim et al. 2010) for production of various kinds of cytokines, including TNF-α, IFN-γ, and IL-1β, and stimulation of NK cells, T and B, which is connected with inhibition of cancer cell growth (Lindequist et al. 2005; Lee et al. 2010). After recognition and attachment of the PS molecule, immune processes such as production of free radicals, phagocytosis, or production of cytokines involved in inflammation are activated (Brown and Gordon 2005; Chan et al. 2009). Chen et al. (2008a, b) showed that EPS from Fomes fomentarius has a direct antiproliferative effect in vitro on SGC-7901 human gastric cancer cell. Crude EPS obtained by Osińska-Jaroszuk et al. (2014) from G. applanatum exhibited antitumor activity against carcinoma cells (lines SiHa) and stimulated the production of Il-6 and TNF-α by the macrophage line THP-1. EPSs produced by Pleurotus sajor-caju act as an anti-inflammatory agent reducing nociception and edema (Silveira et al. 2015). Kim et al. (2010) demonstrated that the cordlan PS isolated from Cordyceps militaris induced phenotypic maturation of dendritic cells demonstrated. Zhang et al. (2010) reported immunomodulatory function and antitumor activity of an EPS fraction EPSF prepared from Cordycepssinensis, which significantly enhanced the Neutral Red uptake capacity of peritoneal macrophages and splenic lymphocyte proliferation in B16-bearing mice and inhibited metastasis of B16 melanoma cells to lungs and livers.

EPS recovered from the culture supernatant of the human pathogenic fungus Cryptococcusneoformans can elicit the immunological response providing convenient source of EPS preparations suitable for immunological studies and of EPS-based vaccines for prevention of cryptococcosis (Datta and Pirofski 2006; Frases et al. 2008; Table 3).

Furthermore, EPS obtained from culture of Cryptococcus laurentii belonging to the same genus seems to be a very promising biotechnological product in wound management, as it significantly improved excisional wound healing in rats in in vitro experiments (Smirnou et al. 2014).

Hypoglycemic, hypolipidemic, and hepatoprotective activities

Several PSs from edible fungi have a proven hypoglycemic effect via a decrease in the glucose level in blood or modulation of glucose/insulin metabolism. A majority of publications on this topic are related to studies of intracellular PSs (Mao et al. 2009). For example, intracellular PS obtained from Ganoderma lucidium decreased fasting serum glucose and insulin levels, and the epididymal fat/BW ratio in type-2 diabetic mice (Xiao et al. 2012) and delayed progression of diabetic renal complications (He et al. 2006). There are also a growing number of reports concerning the ability of some EPSs to reduce glucose levels (Table 3). Cho et al. (2007) reported that EPSs from two different Basidiomycota strains, Tremella fuciformis and Phellinus baumii, exhibited a considerable hypoglycemic effect and improved insulin sensitivity through the regulation of peroxisome proliferator-activated receptor (PPAR)-γ-mediated lipid metabolism. Oral administration of EPS produced by Cerrena unicolor, Coprinus comatus, and Lenzites betulina significantly decreased glucose levels in the serum in streptozotocin-induced diabetic rats (Yamac et al. 2009).

One of the pharmacological properties of fungal EPS is the ability to lower the level of cholesterol and the content of lipids in blood (Table 3). After application of glucan, increased excretion of bile acids and short chain fatty acids was observed. This process inhibits the incorporation of acetate to serum lipids, a substrate required for the synthesis of sterols and fatty acids. This is probably related to the gelling properties of glucans, which also inhibit absorption of cholesterol and triglycerols (Guillamon et al. 2010). Significant reduction of total cholesterol and triglyceride levels in plasma was observed in rats fed with C. militaris and Lentinus edodes EPSs (Yang et al. 2000, 2002). Botryosphaeran, a water-soluble EPS of the β-(1 → 3; 1 → 6)-D glucan type isolated from the culture medium of Botryosphaeria rhodina, administered by gavage, also reduced the plasma levels of total cholesterol and low density lipoprotein-cholesterol in hyperlipidemic rats (Miranda-Nantes et al. 2011). Hypolipidemic and hypoglycemic activities have also been described for EPSs obtained from Ascomycota strains from species C. militaris and B. rhodina cultures (Table 3).

The possible role of EPS in hepatoprotection has also been discussed. For example, the hepatoprotective activity of water extracts containing EPS from Antrodia cinnamomea on ethanol-induced cytotoxicity in AML12 hepatocytes was determined (Ho et al. 2008).

Potential environmental and agricultural applications

The EPS-as potential biofertilizers enhanced mineral solubilization

The mechanisms used by microorganisms for mineral solubilization have been attributed mainly to acidification, exchange reactions, and chelation (Yadav and Tarafdar 2003). It was found that the ability to release nutrients from minerals (weathering) by fungi resulted from the action of fungal EPS in cooperation with organic acids synthesized by fungi, causing precipitation and dissolution of soil minerals through acidification of surrounding hyphae and chelation of different ions (Welch et al. 1999; Rogers and Bennett 2004; Sheng 2005; Rosling et al. 2009; Xiao et al. 2012). Acidic metabolites adsorbed on the EPS surface bind SiO2 ions from silicate minerals, thereby contributing to K+ release in the soil solution (Liu et al. 2006). Fungal EPSs also contain their own acidic constituents, e.g. carboxylic acid, uronic acids, or functional groups enhancing mineral dissolution (Welch et al. 1999). Many saprotrophic fungi producing EPS, including strains from the genera Penicillium (P. simplicissimus, P. giseofulvum, P. radicum) and Aspergillus (A. fumigatus, A. niger), effectively release phosphorus and potassium through degradation of minerals e.g. Ca phosphates, Fe/Al phosphates, mica, montmorillonite, and K-feldspar and belong to a group of phosphate- or potassium-solubilizing microorganisms (PSM, KSM) (Welch et al. 1999; Wakelin et al. 2004; Barroso and Nahas 2005; Sheng 2005; Yi et al. 2008; Smits 2009; Mahapatra and Banerjee 2013b). Penicillium and Aspergillus strains are very often a fungal component of a special kind of tested (lab-stage) biofertilizers like fungal–bacterial and fungal–rhizobial biofilmed biofertilizers (FBBs and FRBs, respectively) (Wakelin et al. 2004; Lian et al. 2008). There are commercial biofertilizers with Penicillium strains e.g. Provide, TagTeam (produced by Philom BIOS; Canada).

EPSs play a key role in formation of biofilm facilitating colonization of soil particles, seeds, and roots systems. The degree of phosphate solubilization increased up to 230 % after the use of biofilm of Penicillium spp., Pleurotus ostreatus, and Xanthoparmeliamexicana in comparison to fungal monocultures (Seneviratne et al. 2008).

EPS as a potential component of bioremediation preparations removing heavy metals and hydrocarbons

Metal biosorption by EPSs involves ionic interactions (e.g. ion exchange, electrostatic interaction) and physical entrapments (Breierová et al. 2002; Da Silva et al. 2014). EPSs possess a substantial quantity of functional groups (amine, phosphate, hydroxyl, carboxyl, and urinate), which increase the negative charge of EPSs and their ion exchange properties and flocculation activities, and can coordinate with metal ions (complexation) and form organic precipitation (Breierová et al. 2002; Moon et al. 2006; Abdel-Aziz et al. 2012). Under the presence of heavy metals, EPS is more heterogenic and contains higher amounts of different components and reactive groups than under absence of metal (Breierová et al. 2002). After purification of crude pullulan obtained from Aureobasidium pullulans CH1 strain, when glucose was its only component, no metal (Cu, Fe, Zn, Mn, Pb, Cd, Ni and Cr) biosorption was reported (Radulović et al. 2008). Exopolymers of Hansenula anomala CCY 38-1-22 bound 90 % of the total amount of Cd ions sorbed by this resistant strain, while the sensitive strain of Saccharomyces cerevisiae CCY 21-4-100 accumulated this metal predominantly in the cellular compartments (94 %) (Breierová et al. 2002). The biosorption of Cd and Pb ions on EPS produced by the fungus Colletotrichum sp. contributed to removal of 79 and 98 % of cadmium and lead, respectively, from a solution with the initial concentration of these metals of 100 mg l−1 (Da Silva et al. 2014). Moon et al. (2006) found that each gram of pestan (a specific EPS produced by Pestalotiopsis sp. KCTC 8637) absorbed 120 mg of lead or 60 mg of zinc. Fungal EPSs can be as effective in biosorption as fungal biomass (Moon et al. 2006), and can be used as potential biosorbents for removal of heavy metals from wastewaters. The interaction of a marine isolate of the white-rot fungus Flavodon flavus NIOCC#312 EPS with specific lignin-degrading enzymes (e.g. peroxidases and laccase) appears to help in degradation of toxic organic compounds by breaking down polycyclic aromatic hydrocarbons before their contact with mycelium (Raghukumar et al. 2006).

EPSs as potential biocontrol preparations eliciting plant resistance

In the literature, there are many reports concerning the ability of bacterial EPSs and fungal cell wall PSs to induce plant resistance (Tamm et al. 2011) but the ability of fungal EPSs to induce resistance is still poorly studied. To our knowledge, there are only two reports about fungal EPS acting as an elicitor of systemic plant resistance (Table 3). Li et al. (2014) have shown that an oligosaccharide obtained from the EPS of the endophytic fungus Fusarium oxysporum Dzf17 contributed to an increase in the activity of defense-related enzymes such as phenylalanine ammonia lyase, polyphenoloxidase, and peroxidase in Dioscorea zingiberensis suspension cells and seedling cultures. El Oirdi et al. (2011) have shown that EPS of Botrytis cinerea acts as a suppressor of the jasmonic acid (JA) signaling pathway, induces accumulation of salicylic acid (SA) in tomato, and enhances resistance against the hemibiotrophic pathogen Pseudomonas syringae. The phenomenon of induced systemic plant resistance—systemic acquired resistance (SAR) mediated by a SA-dependent process and induced systemic resistance (ISR) mediated by JA and ethylene (ET) involves elevation of the level of phenylpropanoid pathway metabolites not only at the site of introduction of the elicitor but also in the entire plant, even in tissues distant from the infection site (Walters et al. 2013).

Conclusion

Many research groups conduct studies on the EPSs from Ascomycota and Basidiomycota fungi, considering their potential use in various fields of science and industry. The data described above imply that the current work on fungal EPSs is the tip of the iceberg, and many exciting scientific findings are still to come. While knowledge about the structure of EPSs is becoming increasingly clear, details of the mechanisms of EPS action in various systems are only beginning to be understood. The multifarious properties of EPSs create a possibility of their wide future application in both biotechnology and medicine.

Acknowledgments

This work was partially supported by the National Science Centre (2012/07/B/ST5/01799) the basic funds for maintaining research potential at the Faculty of Biology and Biotechnology of UMCS in Lublin (BS-P-11-010-15-2-03/4/5 and BS-M-11-010-15-2-05).

Abbreviations

Arab

Arabinose

CTAB-PS

Isolation of EPS by cetyltrimethylammonium bromide precipitation

EPS

Exopolysaccharide

ET

Ethylene

FBBs

Fungal–bacterial biofilmed biofertilizers

FRBs

Fungal–rhizobial biofilmed biofertilizers

Fuc

Fucose

Gal

Galactose

Glc

Glucose

GlcA

Glucuronic acid

GPC

Gel permeation chromatography

HPAEC

High performance anion exchange chromatography

IEC

Ion exchange chromatography

IFN

Interferon

IL

Interleukin

ISR

Induced systemic resistance

JA

Jasmonic acid

KSM

Potassium solubilizing microorganisms

Mal

Maltose

Man

Mannose

ME

Malt extract

MG

Monosodium glutamate

MSS

Mineral salt solution

NK-cell

Natural killer cell

PDB

Potato dextrose broth

PE

Potato extract

PPAR

Peroxisome proliferator-activated receptor

PS

Polysaccharide

PSM

Phosphate solubilizing microorganisms

Rha

Rhamnose

SA

Salicylic acid

SAR

Systemic acquired resistance

SEC

Size exclusion chromatography

SEC/MALS

The combination of SEC with multi-angle light scattering analysis (MALS)

TCA

Trichloric acetic acid

TNF

Tumor necrosis factor

VMSM

Vogel minimum salt medium

Xyl

Xylose

YE

Yeast extract

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