Cellulolytic potential of thermophilic species from four fungal orders
© Busk and Lange; licensee Springer. 2013
Received: 9 August 2013
Accepted: 11 August 2013
Published: 19 August 2013
Elucidation of fungal biomass degradation is important for understanding the turnover of biological materials in nature and has important implications for industrial biomass conversion. In recent years there has been an increasing interest in elucidating the biological role of thermophilic fungi and in characterization of their industrially useful enzymes. In the present study we investigated the cellulolytic potential of 16 thermophilic fungi from the three ascomycete orders Sordariales, Eurotiales and Onygenales and from the zygomycete order Mucorales thus covering all fungal orders that include thermophiles. Thermophilic fungi are the only described eukaryotes that can grow at temperatures above 45°C. All 16 fungi were able to grow on crystalline cellulose but their secreted enzymes showed widely different cellulolytic activities, pH optima and thermostabilities. Interestingly, in contrast to previous reports, we found that some fungi such as Melanocarpus albomyces readily grew on crystalline cellulose and produced cellulases. These results indicate that there are large differences in the cellulolytic potential of different isolates of the same species. Furthermore, all the selected species were able to degrade cellulose but the differences in cellulolytic potential and thermostability of the secretome did not correlate to the taxonomic position. PCR amplification and sequencing of 22 cellulase genes from the fungi showed that the level of thermostability of the cellulose-degrading activity could not be inferred from the phylogenetic relationship of the cellulases.
Fungi are important organisms for degradation of plant material in nature. They achieve this by means of secreted enzymes that are stable even under harsh environmental conditions. These same properties make the fungal enzymes suitable for industrial use. One example is fungal cellulases that are deployed in biorefineries for conversion of biomass to fermentable sugars and in the paper, textile and detergent industries (Karmakar and Ray 2011; Kuhad et al. 2011).
The cellulases are classified in the glycoside hydrolase (GH) families (http://www.cazy.org) (Henrissat and Davies 1997). Several different strategies involving many enzyme classes are used in natural degradation of recalcitrant biomass (Dashtban et al. 2009). However, industrial use of cellulases has mainly been focused on endo-1,4-β-D-glucanase and two types of cellobiohydrolases acting respectively from the reducing and from the non-reducing end of the polymer (Banerjee et al 2010). Additional industrially used cellulose-degrading enzymes are β-glucosidases, which degrade β-D-glucose oligomers to glucose and the GH61 proteins, which boost cellulose decomposition by oxidative degradation of the glucose polymer (Harris et al. 2010; Langston et al. 2011; Quinlan et al. 2011; Westereng et al. 2011).
Biomass decomposition by mesophilic fungi has been extensively studied (Dashtban et al. 2009). Whereas enzymes from mesophilic fungi are typically effective at 50°C several thermophilic fungi produce more thermostable enzymes that can be used at temperatures up to 70°C (Murray et al. 2004; Parry et al. 2002; Venturi et al. 2002; Voutilainen et al. 2008; Wojtczak et al. 1987). This high temperature stability is an important asset for industrial use. For example, it has been shown that a mixture of thermostable cellulases exhibits high lignocellulose degrading capacity with a temperature optimum of 65°C (Viikari et al. 2007).
The known thermophilic fungi are either ascomycetes belonging to the orders Sordariales, Eurotiales, and Onygenales or zygomycetes of the order Mucorales (Berka et al. 2011; Morgenstern et al. 2012). These organisms are the only described eukaryotes that can grow at temperatures above 45°C. In nature, thermophilic fungi are typically found in compost, wood chip piles, stored grains, animal dung and other environments that are self-heating due to degradation of plant materials (Johri et al. 1999). Although such material often contains high concentrations of cellulose some thermophilic fungi are poor cellulose-degraders and seem to utilize sugars released by cellulolytic species in the biotope (Maheshwari et al. 2000). Therefore, thermophilic fungi can differ greatly in their cellulolytic potential.
The thermophilic fungus Thermoascus aurantiacus of order Eurotiales has been studied intensively. It grows readily on cellulose (Romanelli et al. 1975) and produces thermostable cellulases and other enzymes (Gomes et al. 2000; Hong et al. 2003; Hong et al. 2007; Khandke et al. 1989; Parry et al. 2001; Parry et al. 2002). One of the interesting enzymes produced by T. aurantiacus is a copper-dependent monooxygenase of the GH61 family (Harris et al. 2010). Several GH61 proteins degrade cellulose by an oxidative mechanism thereby boosting the action of cellulases (Langston et al. 2011; Quinlan et al. 2011; Westereng et al. 2011). The GH61 from T. aurantiacus exhibits high activity in a boosting assay (Harris et al. 2010). The high cellulolytic potential of this fungus is underpinned by the report that extracellular enzymes from T. aurantiacus release the same amount of sugars from pretreated switchgrass as the commercial cellulase blend Cellic Ctec2 (Novozymes, Bagsvaerd, Denmark) at the same protein load (McClendon et al. 2012). In addition to the high activity, the T. aurantiacus enzymes have higher thermostability than Cellic Ctec2, which probably consists mostly of enzymes from mesophilic fungi although the precise composition has not been disclosed by the manufacturer.
Other thermophilic fungi that produce thermostable cellulases are Talaromyces emersonii (Murray et al. 2004; Voutilainen et al. 2010), Myceliophthora thermophila (Roy et al. 1990), Chaetomium thermophilum and Acremonium thermophilum (Voutilainen et al. 2008).
In the present study we investigated the cellulolytic potential of isolates of 16 thermophilic fungi. The fungi were selected from the three ascomycete orders Sordariales, Eurotiales and Onygenales and from zygomycete order Mucorales thus covering all orders which harbor thermophilic fungal species.
All 16 fungi were able to grow on crystalline cellulose but their extracellular enzymes showed widely different cellulolytic activities, pH optima and thermostabilities. Furthermore, we used PCR with degenerate primers to amplify and sequence gene fragments of 22 new cellulases from these fungi. The phylogenetic relationship of the enzymes showed a better correlation to the fungal order than to the thermostability of the fungal cellulose-degrading activity.
Materials and methods
Fungi and growth conditions
List of fungi and growth on cellulose
CBS no. a
Growth on Avicel
Abbreviation used in figs.
Typha, incubated strawand leaf mold
Chicken nest straw
Mushroom compost During peak heating
Saw dust&wood chips In pighouse bedding
Oryza sativa (Gramineae) seeds
Coal spoil tip soil
Decaying Parthenium argentatum
Rotting guayule shrub
Retting Parthenium argentatum
For DNA purification the fungi were grown on 6% wheat bran (Finax, Esbjerg, Denmark), 1.5 % agar (Sigma-Aldrich, Cambridge, UK) plates at the recommended temperature.
Endoglucanase activity was measured with Azo-CM-Cellulose (cat. S-ACMC, Megazyme, Bray, Ireland) as substrate in an assay modified from the manufacturer’s protocol. A culture broth sample of 20 μl was mixed with 20 μl of 2% Azo-CM-Cellulose in 2× McIlvaine Buffer (McIlvaine 1921) at the desired pH. The culture broth sample was incubated at the indicated time and temperature before mixing with 100 μl of precipitant (300 mM Na acetate, 18 mM Zn acetate, 76% EtOH (pH 5)). The stopped reactions were centrifuged 16,000 g for 1 minute and 100 μl of the supernatant was dried down at 80°C and resuspended in 5 μl of water. Finally, the absorption at 600 nm was measured and enzyme activity was calculated as described (Megazyme, Bray, Ireland).
Filter paper assay
Degradation of filter paper was measured by first cutting a 5 × 5 mm piece of filter paper #1 (Whatman, Kent, UK) with a pair of sharp scissors whereafter it was submerged in 80 μl of 1.25x McIlvaine Buffer (McIlvaine 1921) at the desired pH. Next, 20 μl of sample was added and the assay was incubated at the indicated time and temperature. The filter paper was removed and 0.3 μl of Novozym 188 (Novozymes, Bagsvaerd, Denmark) was added and the sample incubated for 30 minutes at 50°C to convert any cellobiose to glucose. The reactions were centrifuged 16,000 g for 1 minute and the supernatant was dried down at 80°C and resuspended in 5 μl of water. Finally, the glucose content of the sample was measured with the D-Glucose HK Assay Kit (Megazyme, Bray, Ireland).
Fungal mycelium was scraped of the top of a wheat bran agar plate, frozen in N2(l) and ground with a mortar and pestle. DNA was extracted from the homogenized mycelium with the Fungal DNA Mini Kit (Omega Bio-Tek, Norcross, GA, USA) according to the manufacturer's instructions.
Fungal mycelium was collected by filtration of liquid cultures through Miracloth (Calbiochem, San Diego, CA, USA) and RNA was purified with a Total RNA kit (A&A Biotechnology, Gdynia, Poland) or with Tri Reagent (Sigma-Aldrich, St. Louis, MO, USA).
Design of degenerated primers
Sequence of conserved peptides and PCR primers
Primer sequence a
The primers were synthesized and HPLC-purified by Sigma-Aldrich (Cambridge, UK).
PCR with degenerated primers
A mix of 100 ng total fungal DNA in 1x Run PCR buffer, 2 mM each dATP, dCTP, dGTP and dTTP, 400 nM forward primer; 400 nM reverse primer; 1U RUN DNA polymerase (A&A Biotechnology, Gdynia, Poland) in a total volume of 20 μl was used for PCR on an MyCycler (Bio-Rad, Hercules, CA, USA) with the following thermal profile:
Initial denaturation 95°C, 5 minutes.
30–40 cycles of 95°C, 20 seconds; annealing temperature, 30 seconds; 72°C, 60 seconds and a final extension at 72°C 5 minutes.
The number of cycles and the annealing temperature was optimized for each primer set (Table 2).
PCR products were analyzed by agarose gel electrophoresis and selected DNA were cut out and purified with the Qiaquick kit (Qiagen, Hilden, Germany).
One μl of the purified PCR product was reamplified in a 50 μl reaction under the same conditions as the original PCR except that only 15 to 20 cycles of PCR were performed.
RT-PCR and RACE
FirstChoice® RLM-RACE Kit (Invitrogen, Grand Island, NY, USA) was used for cDNA synthesis and RACE according to the manufacturer’s protocol.
For RT-PCR 1 μl of the RACE cDNA reaction was used for PCR in a final volume of 20 μl containing 1x Run PCR buffer, 2 mM each dATP, dCTP, dGTP and dTTP, 500 nM forward primer; 500 nM reverse primer; 1U RUN DNA polymerase (A&A Biotechnology, Gdynia, Poland) on an MyCycler (Bio-Rad, Hercules, CA, USA) with the following thermal profile:
Initial denaturation 95°C, 5 minutes.
30 cycles of 95°C, 30 seconds; 60°C, 30 seconds; 72°C, 60 seconds and a final extension at 72°C 5 minutes.
PCR products were analyzed by agarose gel electrophoresis.
Sequencing and analysis
PCR products were cycle sequenced by Eurofins-MWG (Ebersberg, Germany) or StarSEQ (Mainz, Germany) with one of the degenerated primers used for PCR.
The resulting sequences were translated to amino acid sequence and used for BLAST search (Altschul et al. 1997) against the non-redundant protein sequence database at NCBI and inspected for conserved domains (Marchler-Bauer et al. 2011) in the CDD database at NCBI.
P-values were calculated by two-sided Student’s T-test or by analysis of variance tests (ANOVA) unless indicated otherwise.
Nucleotide sequence accession numbers
The DNA sequences of the product of PCR amplification have been deposited in the European Nucleotide Archive databases [EMBL:HG313865, HG313866, HG313868, HG313869, HG313871 - HG313874, HG313876 - HG313881 and HG313883 - HG313889].
To characterize and compare the cellulolytic potential of thermophilic fungi we chose one isolate of each of 16 (according to the provider) non-pathogenic, non-toxin-producing thermophilic fungi.
A medium with microcrystalline cellulose as the only carbon source was inoculated with each of the 16 fungal strains to test their ability to grow on cellulose. All of the fungi could grow on the microcrystalline cellulose. However, Talaromyces leycettanus and T. aurantiacus needed a supplement of 0.5% yeast extract for growth (Table 1). Also Chaetomium senegalense and Talaromyces byssochlamydoides grew better when the cellulose minimal medium was supplemented with yeast extract.
Of the 13 fungi where endoglucanase activity was detected the activity measured in the medium from T. leycettanus was more than five times higher than from M. albomyces (P < 0.001, Student’s T-test), which had the second highest endoglucanase activity of the fungi used in the present study (Figure 1).
The relatively broad pH optima measured for fungi like C. senegalense and T. indicae-seudaticae indicate that these fungi are able to degrade cellulose in environments with different pH values (Figure 2). The broad pH optimum may be due to one enzyme, which is active at several pH values, or to different enzymes with different pH optima. The only fungus among the species studied with highest activity at high pH value was the zygomycete T. indicae-seudaticae.
To access the total cellulolytic potential of the secretome from the 13 fungi with endoglucanase activity we measured the activity of the culture supernatants in a filter paper degradation assay. Degradation of filter paper requires the combined activity of both endo- and exocellulases and is often used as a measure of total cellulolytic potential (Dashtban et al. 2010; Zhang et al. 2009).
The loss of cellulolytic potential of T. leycettanus at 70°C does not correlate with the high thermostability of the endoglucanase activity of this fungus. This suggests that one or more of the cellobiohydrolases, monooxygenases or auxiliary enzymes that are involved in filter paper degradation are heat labile.
For T. leycettanus and the 12 other fungi where the endoglucanase activity was measurable this activity was either higher than the filter paper degrading activity or the filter paper degrading was too low to detect (Figures 2 and 4, P < 0.001, Student’s T-test). This result suggests that the release of cellulose polymers from an insoluble substrate is rate limiting compared to the decomposition of the released cellulose into oligomers. However, the data should be interpreted with care as it is difficult to compare activities measured in different assays towards different substrates.
To determine if the fungi have genes encoding endoglucanases and cellobiohydrolases we designed degenerated primers for PCR amplification of the GH45 endoglucanases and the GH6 and GH7 cellobiohydrolases. With these primers it was possible to amplify and sequence partial genes for six GH6, eight GH7 and eight GH45 from the fungi. All sequences were submitted to the European Nucleotide Archive database except for the GH7 from Rhizomucor miehei that can be found in Additional file 1. Expression of the genes was confirmed by RT-PCR of RNA isolated from fungi cultivated on microcrystalline cellulose medium (data not shown).
Genes encoding GH6, GH7 and GH45 enzymes sequenced in this study or found in GenBank
In the present study we have assessed the cellulolytic potential of isolates of 16 different thermophilic fungi belonging to four orders by checking their growth on microcrystalline cellulose and characterizing their secreted cellulose-degrading enzymatic activities.
All of the fungal strains could grow on microcrystalline cellulose and were therefore able to degrade cellulose. Two of the fungi (T. leycettanus and T. aurantiacus) needed a supplement of yeast extract for growth. Two observations point to that the growth of these two fungi on cellulose was not limited by access to carbon but rather by some other factor that could be provided by the yeast extract. Firstly, yeast extract contains 0.4 g carbon per g (Holwerda et al. 2012). Therefore, the total contribution of non-cellulose carbon from the yeast extract is 0.2%, which will only allow limited growth of the fungi. Secondly, T. aurantiacus only grew poorly and T. leycettanus not at all on cellulose medium when the medium was supplemented with easily fermentable carbon in the form of 1% glucose (data not shown). Therefore it was not the amount of available carbon per se that was growth limiting. In support of this notion, T. leycettanus was very capable of degrading cellulose as the enzyme assays showed that it secreted by far the highest amount of cellulases of all the fungi tested.
Interestingly, the M. albomyces strain, which was isolated from chicken nest straw in Nevada, grew readily on the cellulose medium in contrast to what was previously reported for a strain of M. albomyces isolated from forest soil and compost in India (Maheshwari and Kamalam 1985). This suggests that different isolates of M. albomyces have different cellulolytic potential. Moreover, the M. albomyces strain used in the present study was the fungus with the second highest cellulolytic potential thereby supporting the notion that this strain is able to degrade cellulose in contrast to the previously characterized strain (Maheshwari and Kamalam 1985).
This difference suggests that it is difficult to conclude about growth preferences of a fungal species based on the study of a single strain. It is tempting to speculate that the original biotope of the strain used in the present study had higher cellulose content than the biotope of the strain used by Maheshwari and Kamalam (Maheshwari and Kamalam 1985).
Likewise, T. lanuginosus is generally considered to be unable to utilize cellulose as sole carbon source (Maheshwari et al. 2000) in contrast to the observation in the present study. However, different strains of T. lanuginosus have different ability to grow on cellulose (Markowska-Szczupak et al. 2012) in agreement with that there can be large differences in the cellulolytic potential of different isolates of the same species.
This notion is supported by the absence of detectable endoglucanase activity from the strain of S. thermophilum used in the present study whereas it has been reported that other strains of S. thermophilum produce endoglucanase and other cellulases when grown on recalcitrant polysaccharides (Hayashida and Mo 1986; Ögel et al. 2001; Poças-Fonseca et al. 2000).
It is difficult to account for that some of the fungi e.g. S. thermophilum could grow on cellulose without producing any detectable endoglucanase activity. It cannot be completely ruled out that the cellulose-degrading activity is membrane associated but it is highly unlikely as no endoglucanase activity was detected in the supernatant from homogenized mycelium (data not shown). Furthermore, it is quite unusual for fungal cellulases to be membrane-anchored although it has been reported. One example is a membrane-anchored endoglucanase that was cloned from Phanerochaete chrysosporium (Vanden Wymelenberg et al. 2002). Another possibility is that S. thermophilum uses a different mechanism such as oxidative processes to degrade the cellulose (Arantes et al. 2011; Rineau et al. 2012). However, this fungus can express cellulose-degrading activity (Ögel et al. 2001) and has genes encoding endoglucanases (Takashima et al. 1999).
One purpose of the present study was to elucidate whether it is possible to predict high thermostability from fungal taxonomy. However, there was no obvious correlation between the fungal orders and the thermostability but at genus level the enzymes from the two species of Talaromyces with measurable endoglucanase activity showed high thermostability. As the cellulolytic potential of some of the isolates used in the present study was different from the cellulolytic potential reported for other isolates of the same species (Hayashida and Mo 1986; Maheshwari et al. 2000; Maheshwari and Kamalam 1985; Markowska-Szczupak et al. 2012; Ögel et al. 2001; Poças-Fonseca et al. 2000) it is likely that the thermostability of enzymes may vary between isolates of the same species. However, the high thermostability observed for the enzyme activity from T. emersonii and T. aurantiacus (both Eurotiales) is in agreement with previous reports on these fungi (Gomes et al. 2000; Hong et al. 2003; Khandke et al. 1989; McClendon et al. 2012; Murray et al. 2004; Parry et al. 2002; Romanelli et al. 1975; Voutilainen et al. 2010).
Just like the taxonomy, the predicted protein sequences of the sequenced genes did not exhibit any correlation to the thermostability of the cellulose-degrading activity. Instead the protein sequences grouped largely according to the taxonomic order with a few exceptions. E.g., the GH45 sequences from Corynascus thermophilus did not fall in the same branch of the phylogenetic tree as the other GH45 from Sordariales. Moreover, the GH45 protein from T. aurantiacus shows higher relationship to the protein from M. albomyces from Sordariales than to the protein for the other fungus of the Eurotiales order, T. emersonii. Similar results were found for the DNA sequences of the enzyme-encoding genes (Additional file 2).
One curious result was that no GH6 encoding genes were found in the two fungi of the order Mucorales. Although it is possible that these fungi have some GH6 genes that were simply not found in the present study, it is interesting that another Zygomycota of the Mucorales order, Rhizopus oryzae, is able to degrade cellulose despite the absence of any GH6 gene in its genome (Battaglia et al. 2011).
The high pH optimum of the cellulolytic activity from T. indicae-seudaticae distinguished this fungus from the other fungi. Also a purified glucoamylase from T. indicae-seudaticae has a relatively high pH optimum (Kumar and Satyanarayana 2003) suggesting that this fungus may be adapted to growth in an environment with high pH.
For six of the eight fungi where high activity was measured in both assays the endoglucanase activity was more heat stable than the filter paper degrading activity (Figure 3 and 5, P = 0.012, Student’s T-test). This is in agreement with that more enzymes including endoglucanases are necessary for filter paper degradation than for decomposition of carboxy-methyl cellulose (reviewed by (Dashtban et al. 2010)). In view of this it seems surprising that C. thermophilum exhibited more stable filter paper degrading activity than endoglucanase activity (Figures 3 and 5). This can be explained by the finding that the endoglucanase activity of C. thermophilum measured as μmoles of glucose released per hour was almost 70 times higher than the filter paper degrading activity. Therefore the endoglucanase activity was not rate limiting for the total cellulolytic potential of the fungus.
In conclusion, the results of the present study show that thermophilic fungi of all four orders from where thermophilic species have been described, are able to degrade cellulose. The main differences in cellulolytic potential and thermostability of the secretome do not seem to correlate to the fungal order.
We thank Mette Lange and Morten Nedergaard Grell for constructive and insightful suggestions.
This work was supported by The Danish Strategic Research Council project 2101-08-0041 (BioRef) and by Novozymes A/S.
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