Functional characterization of a Penicillium chrysogenum mutanase gene induced upon co-cultivation with Bacillus subtilis
© Bajaj et al.; licensee BioMed Central Ltd. 2014
Received: 23 January 2014
Accepted: 17 April 2014
Published: 6 May 2014
Microbial gene expression is strongly influenced by environmental growth conditions. Comparison of gene expression under different conditions is frequently used for functional analysis and to unravel regulatory networks, however, gene expression responses to co-cultivation with other microorganisms, a common occurrence in nature, is rarely studied under laboratory conditions. To explore cellular responses of the antibiotic-producing fungus Penicillium chrysogenum to prokaryotes, the present study investigates its transcriptional responses during co-cultivation with Bacillus subtilis.
Steady-state glucose-limited chemostats of P. chrysogenum grown under penillicin-non-producing conditions were inoculated with B. subtilis. Physiological and transcriptional responses of P. chrysogenum in the resulting mixed culture were monitored over 72 h. Under these conditions, B. subtilis outcompeted P. chrysogenum, as reflected by a three-fold increase of the B. subtilis population size and a two-fold reduction of the P. chrysogenum biomass concentration. Genes involved in the penicillin pathway and in synthesis of the penicillin precursors and side-chain were unresponsive to the presence of B. subtilis. Moreover, Penicillium polyketide synthase and nonribosomal peptide synthase genes were either not expressed or down-regulated. Among the highly responsive genes, two putative α-1,3 endoglucanase (mutanase) genes viz Pc12g07500 and Pc12g13330 were upregulated by more than 15-fold and 8-fold, respectively. Measurement of enzyme activity in the supernatant of mixed culture confirmed that the co-cultivation with B. subtilis induced mutanase production. Mutanase activity was neither observed in pure cultures of P. chrysogenum or B. subtilis, nor during exposure of P. chrysogenum to B. subtilis culture supernatants or heat-inactivated B. subtilis cells. However, mutanase production was observed in cultures of P. chrysogenum exposed to filter-sterilized supernatants of mixed cultures of P. chrysogenum and B. subtilis. Heterologous expression of Pc12g07500 and Pc12g13330 genes in Saccharomyces cerevisiae confirmed that Pc12g07500 encoded an active α-1,3 endoglucanase.
Time-course transcriptional profiling of P. chrysogenum revealed differentially expressed genes during co-cultivation with B. subtilis. Penicillin production was not induced under these conditions. However, induction of a newly characterized P. chrysogenum gene encoding α-1,3 endoglucanase may enhance the efficacy of fungal antibiotics by degrading bacterial exopolysaccharides.
KeywordsTime-course transcriptional analysis Mixed culture Chemostat-based transcriptomics Mutanase Heterologous expression Penicillium chrysogenum Bacillus subtilis
Penicillium chrysogenum is widely used for industrial production of β-lactam antibiotics such as penicillins and cephalosporins. Current production strains are the result of classical strain development programmes which, over a period spanning more than six decades, has improved productivity by several orders of magnitude . Throughout strain improvement, industrial and academic research has sought to understand the molecular basis and physiology of penicillin production by P. chrysogenum based on research in pure cultures.
The complete genome sequence of P. chrysogenum revealed 20 putative polyketide synthase genes (PKS), 10 non-ribosomal peptide synthase (NRPS) genes and 2 genes encoding hybrid NRPS-PKS enzymes [3, 4]. Most of these genes are not significantly transcribed under standard laboratory conditions [5–10] and, consequently, their functional and physiological roles remains to be determined.
The contribution of many secondary metabolites to evolutionary fitness of the producing organism remains unknown and subject to debate [11–14]. It is generally assumed that fungal penicillin biosynthesis has primarily evolved as a mechanism to combat competing bacteria. However, there is no evidence that fungal penicillin biosynthesis is triggered by the presence of bacteria. Moreover, there is no a priori reason to assume that synthesis of fungal antibiotics it is single-layer defense mechanism. For example, NRPS or PKS gene clusters may enable the synthesis of compounds that complement and/or augment the action of penicillins.
Several strategies have been successfully applied to activate and characterize cryptic gene clusters in filamentous fungi . These methods include inactivation of biosynthesis genes , heterologous expression  and simulation of conditions that might activate gene clusters in natural environments [5, 6, 18]. A successful example the latter approach was achieved by co-culturing Aspergillus nidulans with Streptomyces hygroscopicus. Genome wide expression analysis of A. nidulans revealed that co-cultivation led to specific expression of a polyketide gene cluster that was silent under standard conditions for laboratory growth of the fungus . This example supports the notion that microbial interactions in natural environments may be a direct trigger for production of secondary metabolites and other means of ‘microbial warfare’. Simulation of these interactions by co-cultivation in the laboratory is therefore a rational strategy to identify natural antimicrobial compounds and mechanisms. Indeed, this approach has been successfully used to study interactions between microorganisms [19–22], allowing the identification of a wide range of responses, ranging from increased production of stress-response related compounds , induction of biofilm formation and modulation of virulence expression . By providing in-depth knowledge on interaction mechanisms it provides an important tool for understanding the physiology of microorganisms, communication between microbial species and drug discovery .
The dynamic nature of microbial interactions in mixed cultures limit the value of static (single time point) gene expression studies. Time-course expression experiments, in which transcriptional responses to an external stimulus are recorded over time  have been applied successfully to a wide range of perturbations [25–29].
The original discovery of penicillin by Fleming was unintentionally based on a co-cultivation experiment, involving interaction of a Penicillium strain with bacteria on solid medium plates . Surprisingly however, interaction of this fungus with prokaryotes has subsequently not been studied in detail. The objective of the present study is to investigate the response of P. chrysogenum to co-cultivation with B. subtilis, a penicillin-sensitive Gram-positive bacterium. To this end, steady-state chemostat cultures of P. chrysogenum Wisconsin 54–1255 were inoculated with B. subtilis. The dynamic transcriptional and physiological responses of P. chrysogenum in the resulting mixed cultures were monitored and analyzed. Several differentially expressed genes potentially reflected responses to the bacterium. To test whether any bacterial signaling molecules are responsible for differential expression of selected fungal genes, P. chrysogenum cultures were supplemented with supernatant of B. subtilis cultures, supernatants from mixed cultures and with heat-inactivated B. subtilis. The specific transcriptional responses, identified using microarray, were verified by analysis of fermentation broth and by functional characterization of selected P. chrysogenum genes in S. cerevisiae.
Co-cultivation of P. chrysogenum and B. subtilis and physiology
Physiological parameters of co-cultivation of P. chrysogenum and B. subtilis
Time elapsed since inoculation with B. subtilis(h)
Total biomass concentrationa(g l-1)
qO2 a,b(mmol g-1 h-1)
qCO2 a,b(mmol g-1 h-1)
4.04 ± 0.11
0.93 ± 0.02
0.85 ± 0.04
4.32 ± 0.07
0.90 ± 0.01
0.81 ± 0.06
4.69 ± 0.17
0.78 ± 0.03
0.75 ± 0.04
4.98 ± 0.29
0.75 ± 0.05
0.71 ± 0.05
Global transcriptional responses of P. chrysogenum to co-cultivation with B. subtilis
Cluster 1 comprises fast-responding genes, which reached 80% of their maximum expression level within the first 24 h. This cluster showed overrepresentation of genes in the MIPS categories involved in primary metabolism, protein synthesis, folding and stabilization, energy conservation, electron transport, respiration and mitochondrial activity (Figure 3). For example, the gene with the highest fold change after 72 h of co-cultivation (+50-fold), Pc12g10440, showed strong similarity to the alternative oxidase aox1 from Aspergillus niger. Cluster 3 contains genes that exhibited slower response profiles and showed an overrepresentation of genes involved in metabolism (Figure 3). In addition to genes with strong similarity to transporters (permeases, maltose transport protein and high-affinity glucose transporter), this category comprised genes with sequence homology to genes encoding carbohydrate cleaving enzymes such as mutanase, mannosidase and alpha-amylase, to a gene encoding a starvation sensing protein (Pc12g13310) and to a gene showing similarity to polyketide synthase PKS17 from Botryotinia fuckeliana (Pc12g13170). Finally, Cluster 4, which comprises genes exhibiting a continuously increasing profile over the 72 h co-cultivation period, showed an overrepresentation of genes involved in cellular import (Figure 3). No fewer than five genes with similarity to the Kluyveromyces lactis high-affinity glucose transporter gene HGT1. (Pc18g00150; Pc21g19660; Pc22g09740 and Pc21g19770) and the glucose transporter rco-3 from Neurospora crassa (Pc12g02080) were found in this cluster (Additional file 1: Table S1).
Transcriptional responses of P. chrysogenum genes involved in secondary metabolite production to co-cultivation with B. subtilis
B. subtilis induced mutanase production in P. chrysogenum
Cloning and functional characterization of two putative P. chrysogenum mutanase genes
Transcript levels of heterologously expressed putative mutanase genes from P. chrysogenum in S. cerevisiae
Gene and S. cerevisiae strain/relevant genotype
Gene expression relative to reference gene ACT1
Pc12g07500 IME208 [pUDE 230 (TDH3 p ::Pc12g07500:: CYC1t)]
1.52 ± 0.16
Pc12g07500 IME209 [pUDE 249 (TDH3 p ::MF(Alpha)1 1–270 -Pc12g07500-∆1–63 ::CYC1 t )]
1.49 ± 0.33
Pc12g13330 IME210 [pUDE 250 (URA3 TDH3 p ::MF(Alpha)1 1–270 -Pc12g13330::CYC1 t )]
1.13 ± 0.08
The absence of mutanase activity in culture supernatants of S. cerevisiae IME208 might originate from a lack of recognition of the Penicillium signal peptide by the yeast secretion machinery. To circumvent this potential problem, the first 63 nucleotides of Pc12g07500 were replaced by the signal peptide of the S.cerevisiae alpha mating factor . The S. cerevisiae strain IME209, expressing the α-factor pre-pro-peptide – P12g07500 chimera, showed a strongly impaired specific growth rate (0.09 ± 0.01 h-1) on glucose synthetic medium. A mutanase activity of 0.03 U.ml-1 was detected in culture supernatants, confirming that Pc12g07500 encodes an active mutanase.
The amino acid sequence analysis of the second putative mutanase gene, Pc12g1330, did not reveal the presence of a signal peptide. Therefore, its cDNA was directly cloned behind the α-factor pre-pro-peptide sequence to promote secretion of the enzyme by S. cerevisiae. In shake flask cultures of the resulting S. cerevisiae strain IME210 on glucose, it showed a specific growth rate of 0.27 ± 0.01 h-1. No mutanase activity was detected in IME210 culture supernatant, despite confirmation by RT-PCR that the gene fusion was transcribed (Table 2).
General responses of P. chrysogenum to co-cultivation with B. subtilis
While co-cultivation experiments under laboratory conditions cannot fully capture the entire complexity of microbial interactions in natural environment, they do enable identification of specific mechanisms by which micro-organisms interact [18, 20–22]. The present study focused on responses of P. chrysogenum to co-cultivation with the B. subtilis. A substantial part of the transcriptional response of P. chrysogenum to co-cultivation could be attributed to competition for glucose, the growth-limiting nutrient used for the chemostat studies. However this has not been experimentally tested since our fermenters were not equipped with rapid sampling port and the actual supernatant sampling procedure was far too long to trust the measured values. When B. subtilis was inoculated in a glucose-limited chemostat of P. chrysogenum, the bacterium was able to grow faster than the fungus and, over a 72 h period, was well on the way to outcompete it highlighting a better affinity (μmax/Ks) of the bacterium for the limited nutrient. The strong up-regulation of P. chrysogenum genes including sugar transporters (Figure 3, Cluster 4), including genes encoding putative high-affinity transporters, represents a typical response of a micro-organism that is confronted with competition for glucose as the growth-limiting nutrient .
The gene Pc12g10440, which showed the strongest upregulation during co-cultivation with B. subtilis, shares strong similarity with the alternative oxidase gene aox1 from A. niger. Alternative oxidases in fungi and plants represent bypass energy coupling sites in the mitochondrial respiratory chain. Their expression is upregulated under a variety of stress conditions, including changes in the supply of, or demand for, carbon, reducing power, and ATP . Interestingly, alternative oxidases have also been directly implicated in the defense against microbes and, in the case of pathogens, with host cells. For example, expression of alternative oxidase in Nicotania attenuata has been shown to contribute to resistance against pathogenic Pseudomonas syringae and, in pathogenic fungi, the enzyme counteracts the host’s immune system [49–51].
The side-chain precursor phenylacetic acid, whose addition is essential for high-level production of penicillin G by P. chrysogenum, was not included in the growth media used for the present study. P. chrysogenum is able to synthesize phenylacetic acid by itself, using L-phenylalanine as a precursor . However, co-cultivation did not affect expression of genes involved in phenylalanine production or catabolism. This result indicated that, at least in this strain background, co-cultivation of a penicillin-sensitive Gram positive bacterium, did not trigger penicillin production. Although the Wisconsin strain of P. chrysogenum represents an early strain in the penicillin strain improvement lineage , we cannot exclude the possibility that its penicillin biosynthetic pathways had already been deregulated as a result of strain improvement, thereby masking induction by the presence of bacterial cells. However, unexpectedly and in contrast to a previous study on co-cultivation of Aspergillus nidulans with Streptomyces hygroscopicus, P. chrysogenum did not induce other secondary metabolite biosynthetic gene clusters upon in response to the presence of B. subtilis (Figure 4).
Expression of fungal mutanase activity results from cross talk between P. chrysogenum and B. subtilis
Although we were unable to connect co-cultivation of P. chrysogenum with a prokaryote to production of low-molecular weight fungal metabolites, co-cultivation clearly triggered the expression of two genes encoding putative α-1, 3 glucanases (Pc12g07500 and Pc12g13330). Synthesis of mutanase (α-1,3-glucanase, EC 22.214.171.124) is induced in several fungi and bacteria when mutan (α-1,3-glucan) or oligosaccharides such as raffinose are present in the growth medium [52–54]. Mutanase production by Trichoderma harzianum is triggered by sugars or molecule with α-1,3 linkages, consistent with the ability of the enzyme to act on α-1,3 linkages in bacterial biofilms and extracellular polysaccharides such as α-mutan .
Upregulation of the putative mutanase genes Pc12g07500 and Pc12g13330 required the presence of the two microorganisms simultaneously. Supernatant of pure B. subtilis culture or heat inactivated B. subtilis cells were not sufficient to induce the expression of these genes (Table 2), suggesting that the triggering molecule(s) is (are) produced by B. subtilis in response to the presence of P. chrysogenum. Induction of the mutanase genes during co-cultivation could, for example, result from the formation of α-1,3 glucan containing exopolysaccharide by B. subtilis in response to co-cultivation by the fungus. This bacterial response could then be countered by the production of mutanase by the fungus. Several pathogenic bacteria in environment reside in exopolysaccharide biofilm which protects bacterial cells from antibiotics . If enzymes produced against these pathogenic bacterial exopolysaccharides in mixed culture enable bacterial biofilm degradation, this might potentiate fungal antibiotics by facilitating access to the bacteria.
P. chrysogenum Pc12g07500 is an atypical fungal mutanase without a mutan binding domain
Pc12g13330, which showed a higher sequence similarity to T. purpurogenus MutA, did not harbor an N terminal sequence corresponding to a signal peptide, but did contain a C-terminal extension corresponding to the mutan binding motif. Of the six P. chrysogenum mutanases, not only Pc12g07500, but also Pc18g06380 missed the α-mutan binding domain. However, in contrast to Pc12g07500, Pc18g06380 did not appear to carry a signal peptide and was not expressed during co-cultivation with B. subtilis.
Hitherto, fungal mutanases have been described as strictly extracellular enzymes [42, 57]. Interestingly, several of the genes with strong sequence similarity to mutanase genes in the P. chrysogenum genome appear to lack excretion signals. 1, 3-α-D-glucan has been detected in cell walls of Aspergilllus wentii and Schizosaccharomyces pombe, intracellular mutanase-like enzymes may play a role in processing and/or degradation of fungal cell wall components. Expression of the P. chrysogenum mutanase gene Pc12g07500 in S. cerevisiae (strain IME209) had a strong negative effect on yeast growth. This is an intriguing observation, since 1,3-α-D-glucan has not been reported to occur in S. cerevisiae cell walls. Detailed analysis of the mode of growth inhibition of mutanase-expressing strains may yield new insights in yeast cell wall composition and biosynthesis.
The present study demonstrates that co-cultivation experiments with defined mixed cultures provide a useful tool for identifying microbial interactions. Under the experimental conditions, B. subtilis successfully competed with P. chrysogenum for the glucose, the growth-limiting nutrient. The fungus did not respond to this competition by induction of pathways for antimicrobial secondary metabolites. However, a co-cultivation-dependent expression of an extracellular fungal mutanase was observed, which was triggered by (an) extracellular compound(s) produced by the mixed cultures but not by pure cultures of the two organisms. Heterologous expression in S. cerevisiae revealed that of the P. chrysogenum genes induced during co-cultivation with B. subtilis encoded an extracellular mutanase that differed from previously described fungal mutanases due to the absence of an α-mutan binding domain.
S. cerevisiae strains used and constructed in this study
MATa SUC2 MAL2-8C ura3-52
MATa SUC2 MAL2-8C
MATa SUC2 MAL2-8C ura3-52 pUDE 230 (URA3 TDH3 p ::Pc12g07500::CYC1 t )
MATa SUC2 MAL2-8C ura3-52 pUDE 249 (URA3 TDH3 p ::MF(Alpha)1 1–270 -Pc12g07500-∆1–63*:: CYC1 t )
MATa SUC2 MAL2-8C ura3-52 pUDE 250 (URA3 TDH3 p ::MF(Alpha)1 1–270 -Pc12g13330:: CYC1 t )
MATa SUC2 MAL2-8C ura3-52 p426GPD (URA3 TDH3 p ::-:: CYC1 t )
Medium composition and preparations
Synthetic medium for growth of P. chrysogenum was prepared as described  and contained, per liter of demineralized water, 8.25 g glucose monohydrate, 0.8 g KH2PO4, 3.5 g (NH4)2SO4, 0.5 g MgSO4.7H2O and 10 ml trace elements solution. The pH was set to 5.5 by addition of 2 M KOH. The trace element solution contained 15 g l-1 Na2EDTA.2H2O, 0.5 g l-1 Cu2SO4.5H2O, 2 g l-1 MnSO4.H2O, 2 g l-1 ZnSO4.7H2O, 4 g l-1 FeSO4.7H2O and 0.5 g l-1 CaCl2.2H2O. The pH of the trace element solution was set at 6.0 by the addition of NaOH. Concentrated medium without glucose was heat autoclaved at 121°C. After media sterilization, a concentrated glucose solution, separately autoclaved at 110°C, was added. For cultivation of B. subtilis, the same medium was used, but with the addition of 50 mM MES and with an initial pH of 6.5. Synthetic medium for growth of S. cerevisiae contained, per liter of demineralized water, 5 g (NH4)2SO4, 3 g KH2PO4, 0.5 g MgSO4.7·H2O and trace elements . Vitamins  were added after heat sterilization of the medium at 120°C for 20 min. Glucose was separately sterilized at 110°C and added to a final concentration of 20 g L-1.
Pure and mixed-culture growth experiments
P. chrysogenum Wisconsin 54–1255 was grown in steady-state, aerobic and glucose-limited chemostat cultures. Chemostat cultures were grown at 25°C in 2 l turbine-stirred bioreactors (Applikon, Schiedam, The Netherlands) with a working volume of 1.8 L, as described previously [5, 6, 62]. In the batch phase a working volume of 1.5 L was maintained. The pH was adjusted to 6.5 and then kept constant at 6.5 through the automatic addition of 2 M NaOH. The bioreactor was sparged with air at a flow rate of 900 ml/min using a Brooks mass-flow controller (Brooks Instruments, Hatfield, PA). Spores immobilized on rice grains were welled in 100 ml sterilized water until the water became dark green. The liquid then was transferred to a new flask and served as inoculum. To protect the germination process the stirrer speed was initially set at 350 rpm. The dissolved-oxygen concentration was continuously monitored with an oxygen electrode (AppliSens, Schiedam, The Netherlands). When dissolved oxygen reached 60% of air saturation, the stirrer speed was increased to 500 rpm and, subsequently, to 750 rpm to keep dissolved oxygen concentration above 50% of air saturation. To prevent excessive foaming, antifoam Silcolapse 5020 (Bluestar Silicones, East Brunswick NJ) was discontinuously added at timed intervals (6 s on, every 7 min, 1.0 ml h-1). The off-gas was cooled using a condenser (4°C) and dried with a Perma Pure dryer (MD-110- 48P-4, Permapure, Toms River, NJ). Concentrations of CO2 and O2 in the off-gas were measured with a NGA 2000 Rosemount analyzer (Rosemount Analytical, Solon, OH). Off-gas flow rate was measured with a SAGA digital flow meter (Ion Science, Cambridge, United Kingdom). The continuous-feed phase was initiated when the CO2 concentration in the off gas reached 0.3%. A dilution rate of 0.03 h-1 was set by continuous addition of fresh medium with a calibrated peristaltic pump (Masterflex, Vernon Hills, IL). To keep the culture volume constant, culture broth was automatically removed at regular time intervals by applying an overpressure to the reactor by a system of valves .
Precultures of B. subtillis were grown by inoculating 1 ml of B. subtilis glycerol stock into 100 ml of glucose synthetic medium. After incubation in an orbital shaker at 30°C and at 200 rpm for 24 h, a volume of 10 ml was inoculated into 200 ml of glucose synthetic medium in a 1-l shake flask and incubated at 30°C (200 rpm). After 24 h of incubation, when the culture had reached exponential phase, cells were separated aseptically by centrifuging for 20 min at 4°C and at 13000 × g, washed twice and re-suspended in 50 ml sterile P. chrysogenum synthetic medium. The resulting cell suspension, containing ca. 1.8 g dry weight B. subtilis biomass was then aseptically added to to a steady-state chemostat culture of P. chrysogenum bioreactor. The resulting mixed culture was then followed for 72 h while samples were taken for analysis of biomass and metabolites, microscopic observations and transcriptome analysis (samples times 5 h, 24 h, 48 h and 72 h after addition of B. subtilis).
Effects of B. subtilis culture supernatant, supernatant from mixed cultures, and heat-inactivated B. subtilis cells and addition of 0.1% mutan (kindly provided by Prof. Malgorzata Pleszczynska, Maria Curie-Sklodowska University, Lublin, Poland), 0.1% pullulan (Megazyme International Wicklow, Ireland) and 0.1% dextran (Megazyme) on P. chrysogenum were checked in shake-flask experiments. P. chrysogenum was grown in 100 ml glucose synthetic medium in 500 ml flask at 25°C, shaken at 200 rpm. Fermentation broth of exponentially growing B. subtilis cultures and culture samples taken from 24 h mixed chemostat cultures were filtered through 0.20 μm filters (Supor-200, 47 mm, Pall Life Sciences, East Hills, NY). 30 ml B. subtilis supernatant and 30 ml of mixed-culture supernatant were added aseptically to different 24-h P. chrysogenum cultures. Effects of addition of mutan, pullulan and dextran on mutanase induction in P. chrysogenum were checked in shake-flask experiments. The strain was grown in synthetic medium with 0.1% of mutan, 0.1% pullulan or 0.1% dextran. These cultures were allowed to grow for another 72 h, during which samples were taken at 24 h intervals for determining mutanase activity. All cultivation experiments were performed in triplicate.
Heat-inactivated B. subtilis cells were generated by autoclaving 30 ml of exponentially growing B. subtilis culture for 20 min at 121°C. Killed cells were separated aseptically by centrifuging for 20 min at 4°C and at 13000 × g, washed twice and re-suspended in 10 ml of with sterile synthetic medium. The resulting suspension was then aseptically added to a 24-h P. chrysogenum shake-flask culture. Control experiments were performed by using exponentially growing B. subtilis cells instead of killed cells.
Determination of culture dry weight
For P. chrysogenum, 10 ml fermentation broth was filtered over preweighed glass fiber filters Type A/E (Pall Life Sciences). The filters were washed with demineralised water and dried for 20 min at 600 W in a microwave oven and were weighed immediately. For B. subtilis, 10 ml fermentation broth was filtered over preweighed 0.45 μm filters (Supor-450, 47 mm, Pall Life Sciences). The filters were washed with demineralised water and dried for 20 min at 350 W in a microwave oven and were weighed immediately. For mixed cultures, 10 ml of culture sample was filtered over preweighed glass fiber filters. The filters were washed three times with 10 ml of demineralised water so that all the bacterial biomass passed through the glass fiber filters; the combined filtrate was collected. The glass fiber filters were dried for 20 min at 600 W in a microwave oven and were weighed immediately. The collected filtrate was passed through preweighed 0.45 μm filters. The filters were washed with demineralised water and dried for 20 min at 350 W in a microwave oven and were weighed immediately.
Glucose in culture supernatants was analyzed on a Waters 2695 HPLC (Waters, Milford, MA) equipped with an Aminex HPX-87H column (Bio-rad, Hercules, CA) which was coupled to a Waters 2487 dual λ absorbance detector (Waters) at 60°C with 5 mM H2SO4 as the mobile phase. Supernatant was separated from the biomass by filtration using a 0.2 μm filter.
Microscopic observations of the mixed culture were made with a Zeiss Axio imager D1 equipped with an Axio Camera (Carl Zeiss, Jena, Germany).
Mutanase activity was assayed by incubating 0.5 ml of culture supernatant and 0.5 ml of a 0.2% (w/v) suspension of dextranase-treated mutan in 0.05 M potassium phosphate buffer, pH 6.5 at 45°C (kindly provided by Prof. Malgorzata Pleszczynska, Maria Curie-Sklodowska University, Lublin, Poland). After 60-min incubation with shaking, the insoluble mutan was centrifuged (13000 rpm for 5 min) and the released reducing sugars were estimated by the Somogyi-Nelson method  using D-glucose as a standard. One unit of mutanase activity (U) was defined as the amount of the enzyme that catalyzes the release of reducing sugars equivalent to 1 μmol per minute under the experimental conditions .
To isolate P. chrysogenum RNA, mixed-culture samples were filtered through glass fiber filters within seconds, the filter with mycelium was quenched in liquid nitrogen and stored at -80°C until use. Total RNA was extracted by using Trizol reagent and acid-phenol chloroform for RNA extraction and purified by the RNeasy mini kit by Quiagen (Venlo, Netherlands). Quality of the purified RNA was verified by the Agilent 2100 bioanalyzer (Agilent, Santa Clara, CA). To isolate S. cerevisiae RNA, cells were collected by rapid filtration and stored at -80°C until use. Total RNA extraction was performed using acid-phenol chloroform for RNA extraction and 3 M Na acetate as described previously in .
Microarray and transcriptome analysis
Chemostat culture samples (60 ml) were rapidly sampled and filtered over a glass fiber filter (Type A/E, Pall Life Sciences, East Hills, NY). The filter containing the mycelium was immediately wrapped in aluminum foil, quenched in liquid nitrogen and stored at -80°C. Samples were processed as described [5, 6, 8, 10]. Acquisition and quantification of microarray images and data filtering were performed using Affymetrix GeneChip Operating Software (GCOS version 1.2). Arrays were globally scaled to a target value of 100, using the average signal from all probe sets. Arrays were analyzed as previously described . Significant changes in expression of the replicate arrays experiments were assessed statistically by using the software Significance Analysis of Microarray (SAM version 1.21) . Fold change (FC) was set to 2 and false discovery rate to 2%. Transcriptome data analyzed in this study have been deposited at the Genome Expression Omnibus database http://www.ncbi.nlm.nih.gov/geo/) under the accession number GSE53286. Expression data were K-mean clustered using GeneData Expressionist software version 5.0 (Genedata, Basel, Switzerland). Clusters were analyzed for enrichment of MIPS categories, assessed by Fisher’s Exact test employing hypergeometric distribution with a p-value cut-off of 5.10-4 (with Bonferroni correction) .
Cloning and functional characterization of P. chrysogenum genes in S. cerevisiae
Oligonucleotide primers used in this study
MF(Alpha)1 Spe 1-RV
Pc12g07500 Spe 1-FW
Pc12g07500 208 FW
Pc12g07500 208 RW
Pc12g07500 209 FW
Pc12g07500 209 RV
Pc12g13330 210 FW
Pc12g13330 210 RV
3′ FW ACT1
3′ RV ACT1
To facilitate secretion of the mature protein in S. cerevisiae, the signal peptide region in Pc12g07500 was replaced with S. cerevisiae α-factor prepropeptide . The gene fragment coding for Pc12g07500 without signal peptide was PCR amplified using primer pair Pc12g07500 SpeI-FW/Attb Pc12g07500-RV (Table 4) and P. chrysogenum cDNA pool prepared from mRNA isolated from mixed culture sample. S. cerevisiae α-factor prepropeptide cDNA was PCR amplified using primer pair Attb MF(Alpha)1-FW/MF(Alpha)1 SpeI-RV (Table 4) and DNA sample isolated from S. cerevisiae CEN.PK113-7D . Both the PCR products were purified and restricted with SpeI, followed by ligation with T4 DNA ligase. The ligation mixture was used as template to perform PCR using primer pair Attb MF(Alpha)1-FW/Attb Pc12g07500-RV and the target DNA fragment was size-selected and gel purified . The purified PCR product was cloned in pDONR™ 221 in a BP clonase™ reaction to get entry clone pUD288. The obtained entry clone pUD 288 was further recombined in LR clonase™ reaction with the destination plasmid pAG426GPD-ccdb  to get the expression clone pUDE249.
A synthetic gene containing S. cerevisiae α-factor prepropeptide and HA tag with Pc12g13330 (2474 bp) was gene optimized using JCat  and procured from GenScript (Piscataway, NJ). Restriction sites SpeI (upstream) and XhoI (downstream) were introduced in the synthetic gene. The synthetic gene and p426GPD  were restricted with SpeI and XhoI and fragments were recovered from agarose gels with a commercial kit (Zymoclean, Zymo Research). The synthetic gene was ligated into SpeI/XhoI digested p426GPD, resulting in plasmid pUDE250. The expression vector pUDE250 carries Pc12g13330 cDNA placed under the control of the TDH3 promoter.
Transformations of recombination reaction products into competent E. coli JM109 were performed with the Z-Competent E. coli transformation kit (Zymo Research, Orange, CA) and plated on LB media containing either ampicillin (100 mg l-1) or kanamycin (50 mg l-1). The gene sequences in entry clone pUD254 and pUD288 were checked by restriction digestion and DNA sequencing performed at BaseClear, BV (Leiden, The Netherlands).
Plasmids pUDE230, pUDE249, pUDE250 and the URA3-bearing ‘empty vector’ plasmid p426GPD  were transformed into S. cerevisiae CEN.PK113-5D using the lithium acetate protocol . After transformations with the yeast expression plasmid, cells were plated on chemically defined medium. Successful insertion of multicopy plasmids was verified by diagnostic PCR using the primer pairs used for PCR amplification. S. cerevisiae CEN.PK113-5D containing plasmids pUDE230, pUDE249, pUDE250 and p426GPD were designated as IME208, IME209, IME210 and IME211 respectively (Table 3).
Quantitative real time PCR (RT-qPCR)
For preparation of cDNA for RT-qPCR, synthesis of first-stand cDNA was carried out using a QuantiTect reverse transcription kit (Qiagen, Venlo, Netherlands). Total RNA was isolated from shake flasks of S. cerevisiae strains IME208, IME 209 and IME 210 according to the manufacturer’s recommendations. Primers for real-time PCR (Table 4) were designed with Clone Manager 9 (Scientific & Educational Software, Cary, NC). Basic Local Alignment Search Tool (BLAST)  analysis was used to verify that each primer pair was specific for a particular P. chrysogenum gene, and would not cross-react with the S. cerevisiae genome. RT-qPCR assays were carried out using SYBR® Green Jumpstart™ Taq ReadyMix™ (Sigma-Aldrich, St. Louis, MO) in the DNA Engine Opticon™ I system from MJ research™ according to the manufacturer’s instructions. PCR reactions on cDNA template were carried out in triplicate. The results for each growth condition were derived from two independently cultured replicates. Data were analyzed using the Opticon Monitor™ software package version 1.04, calculating Ct values. Melting curves were used to monitor the specificity of the reaction. β-Actin (ACT1) was used as an internal control for sample normalization. PCR reactions on each sample were conducted in triplicate. Data were analyzed by the comparative threshold cycle method .
This project was part of the research programme of the Kluyver Centre for Genomics of Industrial Fermentation, which was sponsored by the Netherlands Genomics Initiative. We are grateful to Prof. Malgorzata Pleszczynska, Maria Curie-Sklodowska University, Lublin, Poland for providing mutan samples.
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