- freely available
Int. J. Mol. Sci. 2012, 13(8), 9584-9598; doi:10.3390/ijms13089584
Abstract: Mutanase (α-(1→3)-glucanase) is a little-known inductive enzyme that is potentially useful in dentistry. Here, it was shown that the cell wall preparation (CWP) obtained from the fruiting body or vegetative mycelium of polypore fungus Laetiporus sulphureus is rich in α-(1→3)-glucan and can be successfully used for mutanase induction in Trichoderma harzianum. The content of this biopolymer in the CWP depended on the age of fruiting bodies and increased along with their maturation. In the case of CWP prepared from vegetative mycelia, the amount of α-(1→3)-glucan depended on the mycelium age and also on the kind of medium used for its cultivation. All CWPs prepared from the individually harvested fruiting body specimens induced high mutanase activity (0.53–0.82 U/mL) in T. harzianum after 3 days of cultivation. As for the CWPs obtained from the hyphal mycelia of L. sulpureus, the maximal enzyme productivity (0.34 U/mL after 3 days of incubation) was recorded for CWP prepared from the 3 week-old mycelium cultivated in Sabouraud medium. Statistically, a high positive correlation was found between the total percentage content of α-(1→3)-glucan in the CWP and the mutanase activity.
Mutanase, α-(1→3)-glucan 3-glucanohydrolase, catalyzes hydrolysis of α-(1→3)-glucoside linkages in streptococcal mutans (water-insoluble and highly branched glucans present in oral biofilms), and α-glucans building the structure of the fungal cell wall. The mutan-degrading enzyme has a high potential as a caries preventive agent, due to its ability to solubilize mutans present in dental plaque as well as denture plaque [1–3]. As an active ingredient in dentifrice preparations and chewing gum, mutanase could become a useful supplement to mechanical cleaning of teeth and dentures with a toothbrush, dental sticks, and dental floss. In addition to their potential usefulness in dentistry as an oral therapeutic agent, α-(1→3)-glucanase might be applicable to investigations of α-(1→3)-glucosidic linkages occurring in fungal cell-wall structures and glucans of certain higher plants. Mutanase obtained in a pure form is a unique tool for studying the chemical structures of these carbohydrates. In addition, the isolation of mutanase gene from the biocontrol agent and their further transfer to a plant genome can result in significant improvement in plant defence against fungal pathogens. For example, Arabidopsis thaliana containing the α-(1→3)-glucanase gene cloned from T. harzianum shows significant resistance to infection by the foliar pathogen Botrytis cinerea . Moreover, various preparations of mutanase have also been successfully used for obtaining fungal protoplasts, improvement of filterability of wine obtained from a grapes infected with the mould B. cinerea, and improvement of filterability and injectability during the secondary and tertiary petroleum recovery by waterflooding [5–7].
The mutanase reported until recently has been inducible in media containing streptococcal mutan. Unfortunately, this biopolymer is not available in bulk quantities due to the pathogenicity of its producers (cariogenic streptococci), the necessity to use complex and expensive media (e.g., beef brain-heart infusion), the multistage production process, low product yields (no more than 2 g/L), and high structural heterogeneity. Substitution of mutan by more available inducers could facilitate commercial-scale mutanase production. An alternative source of α-(1→3)-glucans is the fungal cell wall. We have shown that the cell wall preparation from Laetiporus sulphureus effectively induced mutanase in T. harzianum  and, to the best of our knowledge, this was the first occasion when this material had been used for mutanase production.
L. sulphureus is a polypore fungus belonging to a specific group of wood-decomposing Basidiomycetes growing on deciduous trees. This species is widely distributed in Europe, Asia, and North America . It produces large and strong fruiting bodies which are edible when young, and whose wet biomass sometimes reaches a few kilograms. Moreover, this fungus has long been used in Asian herbal medicine  and is also known as a source of antioxidant, antimicrobial, cytostatic and immunostimulative agents and a producer of HIV-1 reverse transcriptase inhibitors [11–13].
L. sulphureus can also be cultivated on a larger scale in a laboratory both as fruiting bodies in a solid-state surface culture and as a hyphal mycelium in a fermenter submerged culture [14–15]. Moreover, the cell wall of this fungus is the richest source of α-(1→3)-glucans (up to 78% dry matter) . Therefore, a mycelial material of L. sulphureus could represent an inexpensive, easily available, and a human-safe source of an inducer for mutanase production.
The aim of this study was estimation of the α-(1→3)-glucan content in the cell wall and possibilities for application of the harvested fruiting bodies and cultured mycelium of the polypore fungus L. sulphureus as T. harzianum mutanase inducers.
2. Results and Discussion
It is well known that the best mutanase inducer is α-(1→3)-glucan synthesized by cariogenic streptococci or isolated from fungal cell wall . In our previous study, we demonstrated that L. sulphureus fruiting bodies were an excellent source of these inducers [8,18].
Among the three tested preparations, i.e., lyophilized and milled preparation of fresh fruiting bodies of L. sulphureus, cell wall preparation (CWP), and purified α-(1→3)-glucan preparation, the highest mutanase productivity (0.71 U/mL) was obtained on CWP, which was also the best reported in the literature . The use of this inducer is further justified from the economic point of view, since its preparation requires a simple and inexpensive procedure.
However, the CWP from L. sulphureus used for mutanase induction in our previous studies was obtained from a mixture, representing a combination of young and aged basidiocarps. The composition of the preparation was not homogenous, as it contained α-(1→3)-glucan fractions originating from many specimens; hence, the induced mutanase activity resulted from the action of various α-(1→3)-glucans. Therefore, in the present work, individual fruiting bodies were analysed for the amount of α-(1→3)-glucan and its effect on the synthesis of T. harzianum CCM F-340 mutanase. Fruiting bodies of L. sulphureus (16 specimens) harvested from various hosts at different times and in many locations were described and divided into three groups distinguished by their maturity, i.e., an immature fruiting body without the hymenophore (A1–A5), a mature fruiting body with immature spores (B1–B3) and a mature fruiting body with mature spores (C1–C8) (Table 1). This classification was consistent with the amount of α-(1→3)-glucan in the L. sulphureus cell wall, which, as suggested by Jelsma and Kreger , increases along with fruiting body maturation. Our results are in good agreement with these authors. It was found that the amount of α-(1→3)-glucan depended, to a certain extent, on the age of the fruiting bodies. In young specimens (group A), their amount oscillated between 17.3% and 37.6% of dry weight; in group B, these polysaccharides were present at a concentration of 36.5–41%, whereas in the oldest ones (group C), they ranged from 42.8 to 47.8% of dry weight.
The CWPs from the harvested fruiting body specimens were used as inducers of T. harzianum mutanase production (Table 2). All the samples described induced high mutanase activity (at a level of 0.53 to 0.82 U/mL) after 3 days of submerged cultivation in shaken flask cultures. The highest enzyme productivity was obtained on the CWP from specimen C3, and it was by 15% higher than that (0.71 U/mL) obtained on the mixture of various fruiting bodies of L. sulphureus used in the previous studies . Moreover, currently this is the best-reported productivity in the literature. For example, while testing enzyme production by T. harzianum OMZ 779 in fermenter runs, Guggenheim and Haller  obtained an activity of 0.08 U/mL after 155 to 165 h. In shaken flask cultures supplemented with 1% mutan, mutanase activity reached its maximum yield of 0.16 U/mL after 120 h of incubation. Meanwhile, using the same fungal strain, Quivey and Kriger , reached the specific mutanase activity of 0.37 U/mg protein after 4 days in shaken flask cultures. Also, based on Streptomyces chartreusis, Inoue et al.  obtained the maximum mutanase activity of 0.005 U/mL after 3 days in shaken flask cultures. In the case of bacterial mutanases, Pleszczyńska et al.  achieved enzyme activities of 0.35 U/mL and 1.17 U/mg protein in a flask culture of Paenibacillus sp. MP-1 grown for 48 h on CWP from fruiting bodies of L. sulphureus. Meyer and Phaff  obtained up to 0.31 U/mL from Bacillus circulans WL-12 by supplementing the media with whole cells of Schizosaccharomyces pombe or purified α-(1→3)-glucan from Aspergillus niger. Streptomyces KI-8 produced mutanase (0.16 U/mL) when it was cultured on α-(1→3)-glucan isolated from dried fruiting bodies of Lentinus edodes .
As can be seen from the data summarized in Table 2, mutanolytic activity higher than 0.71 U/mL was also obtained on the CWPs from specimens C1, C2, and C5. Moreover, the level of enzyme activity obtained on CWP from the individual specimens was closely related to the amount of α-(1→3)-glucan in the inducer. The correlation was confirmed by statistical analyses (Figure 1). The data obtained from those analyses (Pearson’s correlation coefficient R = 0.776, the coefficient of determination R2 = 0.602, linear regression y = 0.0066x + 0.2844, p < 0.05) indicate a high positive correlation between the content of α-(1→3)-glucan in the CWP and the induced mutanase activity. However, no such correlation was observed after assessment of the enzyme activity per gram of α-(1→3)-glucan used for induction (Table 2). For example, CWP with the lowest content of α-(1→3)-glucan (A1) induced the highest enzymatic activity (3.38 U/g of α-(1→3)-glucan), whereas CWP with the highest content of α-(1→3)-glucan (C5) induced one of the lowest activities (2.51 U/g of α-(1→3)-glucan). Based on these results, it can be supposed that the level of mutanase production depends not only on the amounts of α-(1→3)-glucan, but also on other factors such as the spatial arrangement of linkages in the inducer molecule and the accessibility of enzyme to α-(1→3) sequences.
An attempt was also made to select a culture medium for the production of L. sulphureus mycelium and to investigate the ability of mycelial biomass to induce mutanase. Hyphal mycelium of L. sulphureus can be readily obtained on a large scale. Consequently, mutanase production could become independent of the fruiting bodies, which can be harvested only over limited periods (late spring and early summer). In the experiments described, the strain L. sulphureus CBS 388.61 was cultivated in nine media for up to 5 weeks. The cultures were withdrawn at appropriate intervals (1, 3, and 5 weeks) and the mycelium biomass was measured. We used specific fluorophore-labeled antibodies in order to detect α-(1→3)-glucan in the cell wall of particular mycelium samples. Figure 2 shows a typical image of this staining (L. sulphureus mycelium cultured on medium IV), where α-(1→3)-glucan is clearly labeled in the hyphae. Moreover, a significant accumulation of glucan was observed in hyphal septa.
As shown in Table 3, five culture media yielded over 1 g/L of dry weight of mycelium after 5-week incubation. The maximum biomass production (5.53 g/L) was achieved in Sabouraud medium (IV) after 5-week cultivation. The mycelium production yields in media V, VI, VII, and IX were relatively low; therefore, they were excluded from further study.
The content of α-(1→3)-glucan in water-extracted mycelium (CWP) and non-treated mycelium obtained after 1- to 5-week incubation in 5 selected media was also analyzed (Tables 3, 4). It was found that a 3-week mycelium obtained in Sabouraud medium (IV) contained the highest amount of α-(1→3)-glucan, i.e., 19.7% and 27.8% in non-treated mycelium and CWP, respectively. Apart from one case (specimen A1), the amount of α-(1→3)-glucan in mycelia of L. sulphureus was significantly lower (by ca. 7.2–28.1% and 11.2–45.6% for non-treated mycelium and CWP, respectively) than that isolated from a majority of the fruiting bodies. In general, the content of α-(1→3)-glucan in the mycelia obtained in the nine various media increased and exhibited the highest value after 5-week incubation (Table 3). However, in the case of media IV and VIII, the amount of this biopolymer decreased compared to the 3-week mycelium, which may be explained by cell wall autolysis that starts after exhaustion of external carbon sources and reserve substrates. During this process, lytic enzymes (among others α-(1→3)-glucanase) with activities hydrolyzing the polymers contained in the fungal cell wall are released [25,26]. The fluctuations of mycelium dry weight were also reported by Jaroszuk-Œciseł et al.  for Fusarium culmorum cultivated in a glucose medium. After 42-day incubation, the percentage decrease in the dry weight of mycelium in relation to its maximum dry weight amounted to ca. 20%.
On the other hand, the cause of the reduction in the amount of α-(1→3)-glucan in the mycelium of L. sulphureus may have been the production of spores, whose considerable amounts were detected in the 5-week biomass obtained in medium IV (Figure 3). A study by Grün et al.  indicated that the synthase for vegetative cell wall α-(1→3)-glucan (Ags1p) is downregulated during sporulation, whereas Ags1p homologs for spore wall α-(1→3)-glucan are upregulated. It should be emphasized here that during preparation of CWP from the 5-week L. sulphureus mycelium, the spores were washed away as a result of biomass pre-rinsing and filtering. This resulted in a lower content of α-(1→3)-glucan in the CWP.
The effect of CWPs from mycelia on mutanase production by T. harzianum CCM F-340 is shown in Table 4. Among the five media used in this stage of the research, the CWPs from the mycelium obtained on Sabouraud medium (IV) were the most effective with respect to mutanase productivity. The maximum mutanase yield (0.34 U/mL) was monitored on the CWP from the three-week mycelium. However, it was still about 2.5 times lower than the best activity induced by the CWP derived from fruiting body C3. Nevertheless, it is noteworthy that CWPs derived from both, fruiting bodies and mycelia are in many cases equally efficient as Trichoderma mutanase inducers, especially if we relate the level of enzyme activity to gram of α-(1→3)-glucan content in fungal material (Tables 2, 4). As in the case of induction using the CWP from fruiting bodies, in the case of the CWP from mycelia, we observed a high positive value of the Pearson correlation coefficient (R = 0.908, p < 0.05) and the linear correlation (y = 0.0124x − 0.0637, R2 = 0.8256, p < 0.05) indicated close dependence between the content of α-(1→3)-glucan in CWP and the induced mutanase activity (Figure 4).
The results from the present study have indicated that both the fruiting bodies and mycelium of L. sulphureus may be a valuable source of mutanase inducers. Furthermore, in terms of industrial production, the use of mycelia for efficient mutanase synthesis renders continuous production of the enzyme possible with no need to use seasonally growing fruiting bodies.
3. Experimental Section
The fruiting bodies of Laetiporus sulphureus (Bull.: Fr.) Murrill were harvested from various host trees at different times and in many locations in Poland (Table 1). The specimens were identified by molecular biological analysis of the internal transcribed region (ITS) of the 5.8S rDNA as described below. Voucher specimens are deposited in the Department of Industrial Microbiology, Maria Curie-Skłodowska University, Lublin, Poland. L. sulphureus CBS 388.61 (CBS, Utrecht, The Netherlands) was cultivated in nine liquid media for production of the mycelium. Trichoderma harzianum strain CCM F-340 (Czech Collection of Microorganisms, Brno, Czech Republic) was used as a starting culture for mutanase induction by cell wall material from L. sulphureus.
3.2. Laetiporus sulphureus Cultivation
The culture of L. sulphureus CBS 388.61 was maintained on malt extract agar (MEA) slants (2% malt extract, 1.5% agar), stored at 4 °C and subcultured every month. The seed cultures were grown in 500 mL flasks containing 100 mL of the incubation medium at 25 °C on a rotary shaker incubator at 200 rpm for 7 days. The culture incubation media (500 mL) in 1 L flasks were inoculated with 5% (v/v) of the adequate seed culture and then cultivated for 5 weeks at 25 °C on a rotary shaker incubator at 150 rpm. The composition of the nine different incubation media was described earlier, i.e., medium I by Lamer-Zarawska et al. ; medium II by Davoli et al. ; medium III by Kartal et al. ; medium IV (Sabouraud Liquid Broth) by Baltimore Biological Laboratory, USA; media V-VIII by Jaouani et al. ; medium IX by Sani et al. . Samples of biomass taken after 1, 3, and 5 weeks were centrifuged at 17001 × g for 30 min. After repeated washing with distilled water and drying by lyophilization, the mycelia were used for further analysis.
3.3. Trichoderma harzianum Cultivation
Stock cultures of T. harzianum CCM F-340 maintained at 4 °C on potato dextrose agar slants were used for inoculations. Liquid medium A (pH 5.3), as described by Mandels et al. , supported by 0.4% of CWP (cell wall preparation form L. sulphureus), 0.05% proteose peptone, and 0.1% Tween 80 was used for mutanase production. Shaken cultures were performed in 500 mL conical flasks containing 100 mL of sterile medium. The flasks were seeded with conidia to a final concentration of about 2 × 105 conidia/mL and placed on an orbital rotary shaker at 300 rpm and 30 °C for 3 days.
3.4. Cell Wall and α-(1→3)-Glucan Preparation
The cell wall preparation (CWP) as well as the extraction and purification of α-(1→3)-glucan from fruiting bodies and mycelia of L. sulphureus were performed according to the procedure described by Wiater et al. . The lyophilized fungal material was milled and the resulting powder was treated with water at 121 °C for 1.5 h (× 3). The wall material was removed by centrifugation (17001 × g for 30 min) and freeze-dried (Cell Wall Preparation, CWP). To isolate the alkali-soluble fraction, the CWP was suspended in 1 M NaOH under constant stirring. After overnight-incubation at room temperature, the supernatant was neutralized with 1 M HCl. The insoluble fraction was collected by centrifugation, washed with water (× 3), and lyophilized to give a white powder (purified α-(1→3)-glucan). The polysaccharides obtained were analyzed by FT-IR and 1H NMR to confirm α-(1→3)-glucan purity (data not shown).
3.5. Mutanase Assay
The standard mutanase assay mixture contained 0.5 mL of 0.2% (w/v) a dextranase-pretreated mutan (DTM) in 0.2 M sodium acetate buffer (pH 5.5) and 0.5 mL of the suitably diluted enzyme solution. After 1 h incubation at 45 °C, the reducing sugars released were quantified by the Somogyi-Nelson’ method [34–35]. One unit of mutanase activity (U) was defined as the amount of enzyme hydrolyzing mutan to yield reducing sugars equivalent to 1 μmol of glucose/min, and expressed as units per mL of culture (U/mL). 1 U corresponds to 16.67 nkat.
3.6. Preparation of Dextranase-Pretreated Mutan (DTM)
Dextranase-pretreated mutan (DTM) was prepared (50 U of dextranase/mg of native mutan, pH 6.0, 37 °C, 3 × 24 h) as a substrate for mutanase activity. Native mutan was synthesized from sucrose with the use of a mixture of crude glucosyltransferases of cariogenic S. sobrinus/downei CCUG 21020 (The Culture Collection, University of Göteborg, Sweden) as described previously . Dextranase of Penicillium sp. with an enzyme activity of 12.9 U/mg preparation was purchased from Sigma-Aldrich (St. Louis, MO., USA). The linkage structure of the native and the dextranase-pretreated mutan determined by 1H NMR showed that they were mixed-linkage α-(1→3) and α-(1→6) biopolymers with a greater proportion of α-(1→3) to α-(1→6) linkages, namely, 59.1 and 40.9 mol% for native mutan and 79.8 and 20.2 mol% for DTM, respectively.
3.7. Genomic DNA Isolation, Amplification of ITS Sequences, and DNA Sequencing
The extraction procedure followed the methods of Borges et al.  with minor modifications. Small amounts of fungal mycelium were suspended in a lysis buffer (4 mM spermidine, 10 mM EDTA, 100 mM NaCl, 0.5% SDS, 10 mM β-mercaptoethanol, 40 mM Tris-HCl, pH 8.0) and incubated at 65 °C for 40 min. After incubation, the samples were sequentially extracted with phenol and chloroform, centrifuged for 20 min at 10,000 × g, precipitated with ice-cold ethanol, washed with 70% ethanol, dried and redissolved in TE buffer (1 mM Tris-HCl, 100 mM EDTA, pH 8.0). The purity and concentration of the DNA samples were evaluated using ND-1000 (Nanodrop, USA). Polymerase chain reaction amplifications (PCR) followed the protocol of White et al.  in a final volume of 50 μL. The primers ITS1, ITS2, ITS3, and ITS4 were used for PCR amplification and sequencing of the internal transcribed spacers from the ribosomal genes. The reactions were performed in a TPersonal thermocycler (Biometra, Germany). Amplified PCR products were quantified by gel electrophoresis on a 1% agarose gel stained with ethidium bromide and purified by microfiltration using a Clean-up kit (A&A Biotechnology, Poland). Sequencing was performed by fluorescent dye-terminator chemistry with the automated sequencer ABI 3730 (Applied Biosystems Inc., USA) following the manufacturer’s instructions.
3.8. Immunofluorescent Labeling of α-(1→3)-Glucan
Fluorescently labeled antibodies were used to localize of the α-(1→3)-glucan within the spores and cell wall of L. sulphureus . Fresh biomass of L. sulphureus on Lab-Tek II Chamber slides (Nunc, Rochester, USA) was fixed with 3% (v/v) formaldehyde solution in distilled water at 65 °C for 30 min. The fixed fungal cells were washed three times in PBS buffer (137 mM NaCl, 2.7 mM KCl, 8.1 mM Na2HPO4, 1.5 mM KH2PO4, pH 7.4) before being infiltrated by 1% (v/v) Tween 20 in PBS buffer (PBS-T). To detect the presence of the α-(1→3)-glucan, 150 μL solution of mouse IgM MOPC-104E (0.1 mg/mL in PBS buffer) (Sigma, St Louis, MO, USA) as the primary antibody and 150 μL Alexa Fluor 488 goat anti-mouse IgM (μ-chain specific) (0.1 mg/mL in PBS buffer) (Sigma, St. Louis, MO, USA) as the secondary antibody were used. The samples were incubated with primary antibodies overnight at 4 °C in a wet chamber. Incubation with secondary antibodies was performed as follows: 2 h in dark, at 37 °C. Before observation by fluorescent microscope (Olympus BX 51), the antibody-labeled cells were rinsed three times with PBS buffer. The α-(1→3)-glucan was observed using excitation wavelength at 470/500 nm and emission at 525/550 nm.
3.9. Statistical Analysis
Statistical analysis of the data was performed on three replicates from each treatment. Standard deviations between the values obtained in each experiment were less than 5%. Standard deviations were determined using Microsoft® Excel 2000 (Microsoft Corp., Redmond, Washington, USA). The Pearson correlation coefficient (R), the determination coefficient (R2), and the linear regression (y) were determined (using Microsoft® Excel 2000) to show the direction and strength of the relationship between the amount of α-(1→3)-glucan in CWP and the mutanase activities in the culture fluid of T. harzianum after induction by a particular inductor. Other methodological details are included in the legends of the Tables and Figures.
In conclusion, the L. sulphureus is a common, safe, and easily identified polypore fungus. It can be cultivated (as fruiting bodies or mycelium) or harvested from infected trees. The results obtained suggest that the high content of α-(1→3)-glucan makes the fruiting bodies as well as mycelium of L. sulphureus economic and efficient inducers for large-scale production of microbial mutanases. Moreover, it was found that mycelium used as an inducer was equally effective, which facilitates continuous production of the enzyme without the necessity to use seasonally growing fruiting bodies.
This work was financially supported from funds for science in the years 2008–2012 as the development project (No KB/46/13110/IT1-B/U/08).
- Conflict of InterestThe authors declare no conflict of interest.
- Budtz-Jörgensen, E.; Kelstrup, J. Enzymes as denture cleansers. Eur. J. Oral Sci 1977, 85, 209–215. [Google Scholar]
- Inoue, M.; Yakushiji, T.; Mizuno, J.; Yamamoto, Y.; Tanii, S. Inhibition of dental plaque formation by mouthwash containing an endo-a-1,3 glucanase. Clin. Prev. Dent 1990, 12, 10–14. [Google Scholar]
- Pleszczyńska, M.; Wiater, A.; Jodkowska, E.; Rusyan, E.; Dubielecka, M.; Małkiewicz, K.; Paduch, R.; Walasik, K.; Szczodrak, J. The effects of microbial mutanases on dental plaque aggregation and periodontal parameters. Pol. J. Environ. Stud 2011, 20, 91–96. [Google Scholar]
- Calo, L.; García, I.; Gotor, C.; Romero, L.C. Leaf hairs influence phytopathogenic fungus infection and confer an increased resistance when expressing a Trichoderma α-1,3-glucanase. J. Exp. Bot 2006, 57, 3911–3920. [Google Scholar]
- Balasubramanian, N.; Juliet, G.A.; Srikalaivani, P.; Lalithakumari, D. Release and regeneration of protoplasts from the fungus Trichothecium roseum. Can. J. Microbiol 2003, 49, 263–268. [Google Scholar]
- Villettaz, J.C. Enzymatic Treatment of Wine and Must. In U.S. Patent; 4,439,455, 27; March; 1984. [Google Scholar]
- Gozard, J.P.; Jarry, A.; Luccioni, A. Enzymatic Treatment of Solutions of Polysaccharide Biopolymers. In U.S. Patent; 4,775,632, 4; October; 1988. [Google Scholar]
- Wiater, A.; Szczodrak, J.; Pleszczyńska, M. Mutanase induction in Trichoderma harzianum by cell wall of Laetiporus sulphureus and its application for mutan removal from oral biofilms. J. Microbiol. Biotechnol 2008, 18, 1335–1341. [Google Scholar]
- Vasaitis, R.; Menkis, A.; Lim, Y.W.; Seok, S.; Tomsovsky, M.; Jankovsky, L.; Lygis, V.; Slippers, B.; Stenlid, J. Genetic variation and relationships in Laetiporus sulphureus s. lat., as determined by ITS rDNA sequences and in vitro growth rate. Mycol. Res 2009, 113, 326–336. [Google Scholar]
- Wu, S.; Zorn, H.; Krings, U.; Berger, R.G. Characteristic volatiles from young and aged fruiting bodies of wild Polyporus sulfureus (Bull.:Fr.) Fr. J. Agric. Food Chem 2005, 53, 4524–4528. [Google Scholar]
- Gąsiorowski, K.; Brokos, B.; Lamer-Zarawska, E.; Trocha-Grimshaw, J. Polysaccharides from Laetiporus sulphureus (Basidiomycetes) II. Evaluation of immunostimulative and antitumour activity. Bull. Pol. Acad. Sci. Biol. Sci 1993, 41, 347–352. [Google Scholar]
- Mlinarič, A.; Kac, J.; Pohleven, F. Screening of selected wood-damaging fungi for the HIV-1 reverse transcriptase inhibitors. Acta Pharm 2005, 55, 69–79. [Google Scholar]
- Turkoglu, A.; Duru, M.E.; Mercan, N.; Kivrak, I.; Gezer, K. Antioxidant and antimicrobial activities of Laetiporus sulphureus (Bull.) Murrill. Food Chem 2007, 101, 267–273. [Google Scholar]
- Davoli, P.; Mucci, A.; Schenetti, L.; Weber, R.W.S. Laetiporic acids, a family of non-carotenoid polyene pigments from fruitbodies and liquid cultures of Laetiporus sulphureus (Polyporales, Fungi). Phytochemistry 2005, 66, 817–823. [Google Scholar]
- Ershova, E.; Tikhonova, O.V.; Lur’e, L.M.; Efremenkova, O.V.; Kamzolkina, O.V.; Dudnik, V. Antimicrobial activity of Laetiporus sulphureus strains in submurged culture. Antibiot. Khimioter 2003, 48, 18–22. [Google Scholar]
- Jelsma, J.; Kreger, D.R. Observations the cell-wall compositions of the bracket fungi Laetiporus sulphureus and Piptoporus betulinus. Arch. Microbiol 1978, 119, 249–255. [Google Scholar]
- Wiater, A.; Szczodrak, J.; Pleszczyńska, M.; Próchniak, K. Production and use of mutanase from Trichoderma harzianum for effective degradation of streptococcal mutans. Braz. J. Microbiol 2005, 36, 137–146. [Google Scholar]
- Wiater, A.; Pleszczyńska, M.; Szczodrak, J.; Próchniak, K. α-(1→3)-Glucans from cell wall of Laetiporus sulphureus (Bull.:Fr.) Murrill-isolation, characteristics and application for induction of mutanase synthesis. Biotechnologia 2008, 81, 174–189. [Google Scholar]
- Guggenheim, B.; Haller, R. Purification and properties of an a-(1-3)-glucanohydrolase from Trichoderma harzianum. J. Dent. Res 1972, 51, 394–402. [Google Scholar]
- Quivey, R.G.; Kriger, P.S. Raffinose-induced mutanase production from Trichoderma harzianum. FEMS Microbiol. Lett 1993, 112, 307–312. [Google Scholar]
- Inoue, M.; Egami, T.; Yokogawa, K.; Kotani, H.; Morioka, T. Isolation, identification and some cultural conditions of Streptomyces species that produce water-insoluble polyglucan hydrolase. Agric. Biol. Chem 1975, 39, 1391–1400. [Google Scholar]
- Pleszczyńska, M.; Wiater, A.; Szczodrak, J. Mutanase from Paenibacillus sp. MP-1 produced inductively by fungal α-1,3-glucan and its potential for the degradation of mutan and Streptococcus mutans biofilm. Biotechnol. Lett 2010, 32, 1699–1704. [Google Scholar]
- Meyer, M.T.; Phaff, H.J. Purification and properties of (1→3)-α-glucanases from Bacillus circulans WL-12. J. Gen. Microbiol 1980, 118, 197–208. [Google Scholar]
- Imai, K.; Kobayashi, M.; Matsuda, K. Properties of an α-1,3-glucanase from Streptomyces sp. KI-8. Agric. Biol. Chem 1977, 41, 1889–1895. [Google Scholar]
- Alfonso, C.; Santamaria, F.; Nuero, O.M.; Prleto, A.; Leal, J.A.; Reyes, F. Biochemical studies on the cell wall degradation of Fusarium oxysporum f. sp. lycopersici race 2 by its own lytic enzymes for its biocontrol. Lett. Appl. Microbiol 1995, 20, 105–109. [Google Scholar]
- Santamaria, F.; Nuero, O.M.; Alfonso, C.; Prieto, A.; Leal, J.A.; Reyes, F. Cell wall degradation of Fusarium oxysporum f. sp. lycopersici race 2 by lytic enzymes from different Fusarium species for its biocontrol. Lett. Appl. Microbiol 1995, 20, 385–390. [Google Scholar]
- Jaroszuk-Œciseł, J.; Kurek, E.; Słomka, A.; Janczarek, M.; Rodzik, B. Activities of cell wall degrading enzymes in autolyzing cultures of three Fusarium culmorum isolates: Growth promoting, deleterious and pathogenic to rye (Secale cereale). Mycologia 2011, 103, 929–945. [Google Scholar]
- Grün, C.H. Structure and Biosynthesis of Fungal α-Glucans. Ph.D. Dissertation, Utrecht University, Rome, Italy, March 2003. [Google Scholar]
- Lamer-Zarawska, E.; Trocha-Grimshaw, J.; Gąsiorowki, K.; Królicki, Z.A.; Krzyżanowska, J. Polysaccharides from Laetiporus sulphureus (Basidomycetes) I. Isolation Procedure and Preliminary Chemical Characterization. Bull. Pol. Acad. Sci. Biol. Sci 1993, 41, 339–346. [Google Scholar]
- Kartal, S.N.; Munir, E.; Kakitani, T.; Imamura, Y. Bioremediation of CCA-treated wood by brow-rot fungi Fomitopsis palustris, Coniophora puteana, and Laetiorus sulphureus. J. Wood Sci 2004, 50, 182–188. [Google Scholar]
- Jaouani, A.; Sayadi, S.; Vanthournhout, M.; Penninckx, M.J. Potent fungi for decolourisation of oil mill wastewaters. Enzym. Microb. Technol 2003, 33, 802–809. [Google Scholar]
- Sani, R.K.; Banerjee, U.C. Decolorization of triphenylmethane dyes and textile and dye-stuff effluent by Kurthi sp. Enzyme Microb. Technol 1999, 24, 433–437. [Google Scholar]
- Mandels, M.; Parrish, F.W.; Reese, E.T. Sophorose as an inducer of cellulase in Trichoderma viride. J. Bacteriol 1962, 83, 400–408. [Google Scholar]
- Somogyi, M. A new reagent for the determination of sugars. J. Biol. Chem 1945, 160, 61–68. [Google Scholar]
- Nelson, N. A photometric adaptation of the Somogyi method for the determination of glucose. J. Biol. Chem 1944, 153, 375–380. [Google Scholar]
- Wiater, A.; Szczodrak, J.; Pleszczyńska, M. Optimization of conditions for the efficient production of mutan in streptococcal cultures and post-culture liquids. Acta Biol. Hung 2005, 56, 137–150. [Google Scholar]
- Borges, M.I.; Azevedo, M.O.; Bonatelli, J.R.; Felipe, M.S.S.; Astolfi-Filho, S. A practical method for the preparation of total DNA from filamentous fungi. Fungal Genet. Newsl 1990, 37, 2–41. [Google Scholar]
- White, T.J.; Bruns, T.; Lee, S.; Taylor, L. Amplification and direct sequencing of fungal ribosomal RNA genes for phylogenetics. In PCR protocols: A Guide to Methods and Applications; Innis, M.A., Gelfand, D.H., Sninsky, J.J., White, T.J., Eds.; Academic Press: New York, NY, USA, 1990; pp. 315–322. [Google Scholar]
- Fujikawa, T.; Kuga, Y.; Yano, S.; Yoshimi, A.; Tachiki, T.; Abe, K.; Nishimura, M. Dynamics of cell wall components of Magnaporthe grisea during infectious structure development. Mol. Microbiol 2009, 73, 553–570. [Google Scholar]
|Specimen||GenBankaccession NO.||Geographicorigin||Host tree||Fruiting body sizeª||Fruiting body maturityb||α-(1→3)-Glucan(%)c|
|A1||HM245764||Lublin(51°13′N, 22°33′E)||Prunus cerasus||+||+||17.3 ± 0.8|
|A2||HM245765||Piaseczno(52°03′N, 21°00′E)||Salix alba||+++||+||26.9 ± 1.3|
|A3||HM245763||Łomża(53°10′N, 22°03′E)||S. alba||++||+||28.0 ± 1.2|
|A4||HM245772||Warszawa(52°13′N, 21°00′E)||Salix caprea||+++||+||36.2 ± 0.9|
|A5||HM245770||Lublin(51°13′N, 22°33′E)||S. alba||+||+||37.6 ± 1.1|
|B1||HM245771||Węgorzewo(54°12′N, 21°44′E)||Quercus robur||++||++||36.5 ± 0.5|
|B2||HM245766||Lublin(51°13′N, 22°33′E)||S. alba||+||++||37.0 ± 1.4|
|B3||HM245768||Gęś(51°42′N, 23°00′E)||Prunus avium||+++||++||41.0 ± 1.5|
|C1||HM245761||Lublin(51°13′N, 22°33′E)||Fraxinus excelsior||++||+++||42.8 ± 1.3|
|C2||HM245762||Drobin(52°44′N, 19°59′E)||Salix chrysocoma||++||+++||44.7 ± 1.9|
|C3||HM245759||Lublin(51°13′N, 22°33′E)||S. chrysocoma||++||+++||46.4 ± 1.8|
|C4||HM245760||Frampol(50°40′N, 22°40′E)||S. alba||+++||+++||46.7 ± 2.1|
|C5||HM245758||Kurów(51°23′N, 22°11′E)||S. caprea||+++||+++||46.9 ± 0.8|
|C6||HM245774||Bytów(54°10′N, 17°29′E)||Q. robur||++||+++||46.9 ± 1.7|
|C7||HM245767||Zielona(50°59′N, 22°40′E)||P. cerasus||+||+++||47.0 ± 1.1|
|C8||HM245773||Legionowo(52°24′N, 20°55′E)||Robinia pseudoacacia||++||+++||47.8 ± 0.7|
aFruiting body size: (+) < 20 cm, (++) 20–35 cm, (+++) > 35 cm;bFruiting body maturity: (+) immature fruiting body (lack of hymenophore), (++) mature fruiting body with immature spores, (+++) mature fruiting body with mature spores;cAmount of α-(1→3)-glucan in fruiting body dry mass. Results are shown as mean ± SD of three independent experiments.
|Specimen||α-(1→3)-Glucan (%)||U/mL||U/g α-(1→3) Glucan|
|A1||39.4 ± 0.8||0.534 ± 0.025||3.388 ± 0.112|
|A2||50.4 ± 1.9||0.636 ± 0.028||3.155 ± 0.098|
|A3||48.3 ± 1.3||0.625 ± 0.013||3.235 ± 0.052|
|A4||56.8 ± 2.1||0.643 ± 0.009||2.830 ± 0.121|
|A5||57.2 ± 1.6||0.634 ± 0.030||2.771 ± 0.046|
|B1||56.8 ± 1.9||0.636 ± 0.007||2.799 ± 0.077|
|B2||57.0 ± 1.7||0.660 ± 0.015||2.895 ± 0.133|
|B3||60.0 ± 1.1||0.687 ± 0.025||2.863 ± 0.135|
|C1||64.6 ± 2.2||0.718 ± 0.015||2.779 ± 0.127|
|C2||65.8 ± 1.5||0.816 ± 0.019||3.100 ± 0.037|
|C3||67.2 ± 1.7||0.822 ± 0.023||3.058 ± 0.121|
|C4||65.2 ± 1.2||0.702 ± 0.005||2.692 ± 0.099|
|C5||73.4 ± 2.2||0.739 ± 0.029||2.517 ± 0.078|
|C6||69.0 ± 1.7||0.708 ± 0.013||2.565 ± 0.067|
|C7||65.0 ± 1.3||0.610 ± 0.017||2.346 ± 0.111|
|C8||51.4 ± 0.9||0.623 ± 0.015||3.030 ± 0.135|
aSubmerged cultures were performed on modified Mandels’ A medium with 0.4% CWPs in 500 mL conical flasks, each containing 100 mL of the medium. Initial medium pH was 5.3. Results are shown as mean ± SD of three independent experiments.
|Medium||Biomassyield (g/L)||α-(1→3)-Glucan (%)a||Biomassyield (g/L)||α-(1→3)-Glucan (%)a||Biomassyield (g/L)||α-(1→3)-Glucan (%)a|
|I||1.26 ± 0.054||4.7 ± 0.17||2.82 ± 0.097||11.0 ± 0.36||3.40 ± 0.096||12.4 ± 0.19|
|II||0.08 ± 0.004||2.3 ± 0.05||0.58 ± 0.020||5.8 ± 0.16||1.01 ± 0.032||15.1 ± 0.35|
|III||1.35 ± 0.037||7.4 ± 0.15||3.52 ± 0.081||8.2 ± 0.24||5.26 ± 0.156||13.1 ± 0.42|
|IV||1.44 ± 0.034||4.0 ± 0.09||3.75 ± 0.135||19.7 ± 0.55||5.53 ± 0.138||17.9 ± 0.54|
|V||0.02 ± 0.001||n.d.||0.05 ± 0.002||n.d.||0.05 ± 0.002||n.d.|
|VI||0.04 ± 0.002||n.d.||0.05 ± 0.002||n.d.||0.05 ± 0.002||n.d.|
|VII||0.01 ± 0.001||n.d.||0.02 ± 0.001||n.d.||0.03 ± 0.001||n.d.|
|VIII||1.68 ± 0.055||7.3 ± 0.23||2.39 ± 0.051||10.5 ± 0.21||2.85 ± 0.130||7.6 ± 0.21|
|IX||0.07 ± 0.002||n.d.||0.18 ± 0.005||n.d.||0.21 ± 0.011||n.d.|
aAmount of α-(1→3)-glucan in mycelium dry mass. Results are shown as mean ± SD of three independent experiments.n.d.: not detected.
|Source||α-(1→3)-Glucan (%)||U/mL||U/g α-(1→3)-Glucan|
|1 week-old mycelium on medium:|
|I||8.0 ± 0.23||0.063 ± 0.003||1.969 ± 0.058|
|II||4.3 ± 0.11||0.034 ± 0.001||1.976 ± 0.034|
|III||13.2 ± 0.32||0.030 ± 0.001||0.568 ± 0.020|
|IV||7.0 ± 0.21||0.063 ± 0.002||2.250 ± 0.087|
|VIII||12.0 ± 0.34||0.067 ± 0.003||1.396 ± 0.060|
|3 week-old mycelium on medium:|
|I||16.2 ± 0.45||0.109 ± 0.004||1.682 ± 0.048|
|II||12.6 ± 0.24||0.074 ± 0.002||1.468 ± 0.066|
|III||15.6 ± 0.55||0.106 ± 0.003||1.699 ± 0.080|
|IV||27.8 ± 0.51||0.341 ± 0.011||3.067 ± 0.092|
|VIII||15.4 ± 0.33||0.119 ± 0.004||1.932 ± 0.056|
|5 week-old mycelium on medium:|
|I||17.4 ± 0.53||0.115 ± 0.003||1.652 ± 0.052|
|II||22.0 ± 0.81||0.186 ± 0.006||2.114 ± 0.085|
|III||16.8 ± 0.47||0.129 ± 0.005||1.920 ± 0.086|
|IV||25.8 ± 0.88||0.293 ± 0.009||2.839 ± 0.125|
|VIII||12.0 ± 0.48||0.114 ± 0.003||2.375 ± 0.052|
aSubmerged cultures were performed on modified Mandels’ A medium with 0.4% CWPs in 500 mL conical flasks, each containing 100 mL of the medium. Initial medium pH was 5.3. Results are shown as mean ± SD of three independent experiments.
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