High external pH enables more efficient secretion of alkaline α-amylase AmyK38 by Bacillus subtilis
- Kenji Manabe†1, 2,
- Yasushi Kageyama†1,
- Masatoshi Tohata1,
- Katsutoshi Ara1,
- Katsuya Ozaki1Email author and
- Naotake Ogasawara2Email author
© Manabe et al.; licensee BioMed Central Ltd. 2012
Received: 1 March 2012
Accepted: 8 June 2012
Published: 8 June 2012
Bacillus subtilis genome-reduced strain MGB874 exhibits enhanced production of exogenous extracellular alkaline cellulase Egl-237 and subtilisin-like alkaline protease M-protease. Here, we investigated the suitability of strain MGB874 for the production of α-amylase, which was anticipated to provoke secretion stress responses involving the CssRS (Control secretion stress Regulator and Sensor) system.
Compared to wild-type strain 168, the production of a novel alkaline α-amylase, AmyK38, was severely decreased in strain MGB874 and higher secretion stress responses were also induced. Genetic analyses revealed that these phenomena were attributable to the decreased pH of growth medium as a result of the lowered expression of rocG, encoding glutamate dehydrogenase, whose activity leads to NH3 production. Notably, in both the genome-reduced and wild-type strains, an up-shift of the external pH by the addition of an alkaline solution improved AmyK38 production, which was associated with alleviation of the secretion stress response. These results suggest that the optimal external pH for the secretion of AmyK38 is higher than the typical external pH of growth medium used to culture B. subtilis. Under controlled pH conditions, the highest production level (1.08 g l-1) of AmyK38 was obtained using strain MGB874.
We demonstrated for the first time that RocG is an important factor for secretory enzyme production in B. subtilis through its role in preventing acidification of the growth medium. As expected, a higher external pH enabled a more efficient secretion of the alkaline α-amylase AmyK38 in B. subtilis. Under controlled pH conditions, the reduced-genome strain MGB874 was demonstrated to be a beneficial host for the production of AmyK38.
Keywordsα-Amylase AmyK38 Bacillus subtilis CssRS Genome reduction HtrA HtrB MGB874 Secretion stress response
Bacillus subtilis is a Gram-positive sporiferous bacillus with numerous attractive characteristics for the production of industrially important enzymes, including high growth rate, protein secretion ability, and Generally Regarded as Safe (GRAS) status [1–4]. B. subtilis has also been extensively characterized by biochemical, genetic, and molecular biological studies, and the complete sequencing of the B. subtilis strain 168 genome has facilitated genetic engineering of this model organism [5, 6]. Recently, we constructed a series of multiple-deletion mutant strains by the sequential deletion of 865 genes (874 kb; 20.7% of total genomic DNA), including all prophage and prophage-like sequences, the pks and pps operons, and 11 non-essential gene clusters, from B. subtilis strain 168 [7, 8]. One of the generated mutants, strain MGB874, showed enhanced production of exogenous extracellular alkaline cellulase Egl-237  and a subtilisin-like alkaline protease M-protease , which were expressed from a multi-copy plasmid. We demonstrated that two factors contribute to the high enzyme production in reduced-genome strain MGB874: increased specific productivity and improved cell yields . The former is likely attributable to higher target gene expression due to increased promoter activity and plasmid copy number, while the latter may result from an increased supply of glutamate by enhanced glutamate metabolism due to deletion of the rocDEF-rocR region. Therefore, strain MGB874 would be a suitable host for the high-level production of other beneficial industrial enzymes.
α-Amylase (α-1,4-glucan-4-glucanohydrolase, EC22.214.171.124) is an important enzyme in the food and detergent industries. We previously isolated a novel α-amylase, AmyK38 (55,097 Da), from alkaliphilic Bacillus sp. strain KSM-K38 and demonstrated this enzyme has several unique properties, including high activity at alkaline pH and strong resistance to chemical oxidants . In addition, although α-amylases are generally metalloenzymes that contain at least one activating and stabilizing Ca2+ ion , AmyK38 does not associate with Ca2+ ions; rather, its enzyme activity depends on Na+ ions and is not inhibited by chelating reagents. Due to these characteristics, AmyK38 would likely be an advantageous component of laundry and dishwashing detergents, which are alkaline solutions and typically contain bleach and chelating agents. However, the improvement of AmyK38 production levels is a necessary prerequisite for the commercial use of this α-amylase, which is only produced by strain KSM-K38 at markedly low levels (30 mg l-1) .
In B. subtilis, the overproduction of α-amylases from Bacillus licheniformis (AmyL) and Bacillus amyloliquefaciens (AmyQ) provokes a CssRS (Control secretion stress Regulator and Sensor) dependent secretion stress response [14, 15], which represents a significant bottleneck for high-level enzyme production [16, 17]. The misfolded or aggregated forms of AmyL and AmyQ at the membrane-cell wall interface is thought to be detected by the membrane sensor protein CssS , which then activates the response regulator CssR through phosphorylation. Consequently, activated CssR leads to increased transcription of htrA and htrB, which encode putative membrane-bound proteases . Previous studies have shown that inactivation of the dlt operon, which is involved in the D-alanylation of cell wall teichoic acids, leads to the stabilization and increased production of AmyQ in B. subtilis, likely due to increased negative charge density in the cell wall . Furthermore, the inactivation of dlt operon led to a strongly reduced AmyQ-induced secretion stress response as compared to the wild-type strain .
Hagihara et al.  reported that the amino acid sequence of AmyK38 exhibits moderate overall identity with AmyL (62.8%) and AmyQ (59.5%). However, it is not clear whether the overproduction of AmyK38 provokes a secretion stress response in B. subtilis. Here, we investigated the production and secretion stress levels of AmyK38 in genome-reduced strain MGB874.
Results and discussion
Genome reduction significantly decreases production of AmyK38
Investigation of the bottleneck in AmyK38 production in genome-reduced strains
We next examined the concentration of AmyK38 in culture supernatants and cell fractions by Western blotting. As shown in Figure 2B, the levels of AmyK38 in the supernatants decreased in the order of strains 168, MGB625, MGB723, and MGB874, which closely correlated with the α-amylase activities measured at 48 h (Figure 1). Additionally, the levels of AmyK38 detected in the cellular fraction in the genome-reduced strains were also lower than that of strain 168 (Figure 2B). As the size of AmyK38 observed in the cellular fraction was equivalent to that of purified (mature) AmyK38, these cell-associated AmyK38 would be translocated mature protein that has not yet been released into the growth medium. The isoelectric point (pI) of AmyK38 is 4.2 , and AmyK38 we detected in cellular fraction could not be removed by washing with 5 M LiCl (data not shown), suggesting that it is not bound to cell wall, but bound to cell membrane.
To investigate the possible degradation of secreted AmyK38 in the genome-reduced strains, we evaluated the stability of mature AmyK38 in culture medium following the growth of strains 168 and MGB874 harboring pHYK38 to the stationary phase (at 48 h). As shown in Figure 2C, AmyK38 was stable in the spent culture medium of both strains over an incubation period of 24 h at 30°C. This finding indicates that following the folding of AmyK38 into its native conformation and release from the cells into the growth medium, the enzyme is highly stable.
Finally, we measured the transcriptional levels of htrA and htrB, which encode membrane-bound proteases that respond to secretion stress in B. subtilis. The data shown in Figure 2D indicates that the secretion stress levels resulting from the overproduction of AmyK38 were higher in strains MGB723 and MGB874 than those in strains 168 and MGB625. Westers et al.  have demonstrated that the intensity of the secretion stress response in B. subtilis correlates with the cellular level of AmyQ. However, in the present study, the concentration of AmyK38 in the cellular fraction of strains MGB723 and MGB874 was inversely related to the levels of secretion stress, although the amount of cell-associated AmyK38 was also reduced in MGB625 without induction of HtrA and HtrB.
These findings raise the possibility that unfolded forms of AmyK38 accumulated after translocation and they were degraded rapidly at the membrane-cell wall interface in strains MGB723 and MGB874. It was reported that the predominant proteases responsible for protein degradation at the membrane-cell wall interface are the WprA-derived cell wall-bound protein CWBP52  and CssRS-dependent membrane bound proteases HtrA and HtrB . However, the gene encoding WprA was deleted during the multiple deletion process used to construct strains MGB723 and MGB874 [7, 8]. Thus, the main proteases responsible for the degradation of AmyK38 before its release into the growth medium appear to be HtrA and HtrB. In an attempt to confirm this speculation, we evaluated AmyK38 production in cssRS mutants, but no transformants harboring pHYK38 for AmyK38 production could be obtained. This result is consistent with previous reports that found inactivation of cssRS causes growth defects under secretion stress conditions and does not improve the yield of heterologous proteins .
Genetic cause for decreased AmyK38 production
To determine the underlying genetic cause for the significant decrease in AmyK38 production in the genome-reduced strains, we examined the regions deleted during the generation of strain MGB723 from strain MGB625, which involved deletion of the genomic region from pdp to rocR (nucleotides 4,049,059 to 4,147,133 in sequence NC_000964.3; NCBI GenBank Database ). Deletion of this genomic region significantly increased the production of cellulase Egl-237 and M-protease [7, 8], with subsequent analyses revealing that deletion of the rocDEF-rocR region was responsible for the enhanced enzyme production . However, here, we found that deletion of the rocDEF-rocR region caused a significant decrease in the production level of AmyK38 (Additional file 1: Figure S1). Thus, deletion of the rocDEF-rocR region has a negative effect on the production of the α-amylase AmyK38, but leads to increased production of Egl-237 and M-protease .
RocG is a catabolic glutamate dehydrogenase that catalyzes the conversion of glutamate to 2-oxoglutarate and ammonia . As the deamination of glutamate by RocG is a major ammonia-releasing reaction , which would lead to increased external pH, we focused on ammonia generation and changes in external pH of the culture medium (Figure 4C). We found that the ammonia concentrations in the growth media and external pH were higher under rocG- induced conditions compared to those measured under non-inducing conditions. In the non-inducing conditions, the production of AmyK38 was arrested in the stationary phase (Figure 4A, white bars, 24 to 48 h). During this growth phase, the external pH was lower (Figure 4C) and the secretion stress levels were higher (Figure 4B) compared to those detected under inducing conditions. Together, these data suggest the possibility that a lower pH leads to decreased extracellular production of AmyK38, which is accompanied by increased levels of secretion stress in B. subtilis. At 72 h of cultivation, the external pH for strain MGB874 was drastically increased, likely due to sugar starvation (Figure 4D) . In accordance with this increase in external pH, the production of AmyK38 increased from 48 to 72 h of cultivation under non-inducing conditions of rocG (Figure 4A).
Up-shift in external pH enhances AmyK38 production levels and decreases secretion stress
Effect of pH up-shift on the secretion stress response in B. subtilis
168 ΔamyE::P htrB -lacZ
6.7 ± 0.3
168 ΔamyE::P htrB -lacZ
6.5 ± 0.5
MGB874 ΔamyE::P htrB -lacZ
9.5 ± 0.1
MGB874 ΔamyE::P htrB -lacZ
9.1 ± 0.3
168 ΔamyE::P htrB -lacZ
700 ± 86
168 ΔamyE::P htrB -lacZ
200 ± 48
MGB874 ΔamyE::P htrB -lacZ
1700 ± 36
MGB874 ΔamyE::P htrB -lacZ
590 ± 85
To further improve AmyK38 production, we attempted to reduce the remaining secretion stress response by further increasing the external pH (Figure 5A, 1.2% Na2CO3 [w/v]). Increasing the external pH from pH 8.4 to 9.1 resulted in a decrease in the culture OD600 at 24 h of cultivation. Under this cultivation condition, the culture OD600 of strain MGB874 remained low until the end of the 72 h cultivation period, whereas increases in the culture OD600 of strain 168 were observed after only 24 h of cultivation. Thus, the severe growth inhibition of strain MGB874 cells would result in drastically decreased AmyK38 production (Figure 5A, 1.2% Na2CO3 [w/v]). Therefore, further enhancement of AmyK38 production is expected by the generation of a high alkaline-tolerant mutant of strain MGB874.
Reduced D-alanylation enhances production of AmyK38 in response to external pH up-shift
Under normal growth conditions (pH 6.5), cell wall teichoic acids of B. subtilis contain ester-linked D-alanine residues, which reduce the density of negative charge in the cell wall . Hyyrylainen et al.  reported that a D-alanylation-deficient strain (ΔdltB) displays increased α-amylase production compared to the wild-type strain . Importantly, under alkaline conditions (pH 8.1), cell wall teichoic acids are non-alanylated due to the lability of D-alanine ester linkages at alkaline pH . These observations suggest that the enhanced production of AmyK38 in response to an external pH up-shift might be due to the loss of D-alanine esters under alkaline conditions. Thus, we constructed D-alanylation-deficient mutants (ΔdltB) of strains 168 and MGB874, and then evaluated the production levels of AmyK38 in the presence and absence of added alkali.
AmyK38 production in dltB mutants with or without an up-shift of external pH
α-amylase activity(kU l-1)b
2.9 ± 0.3
7.0 ± 0.3
0.10 ± 0.01
0.27 ± 0.02
14.3 ± 0.2
14.8 ± 0.4
20.8 ± 0.8
20.1 ± 0.2
In summary, the observed improvement of AmyK38 production by B. subtilis in response to an up-shift of external pH is considered to be a result of the following: (i) direct improvement of the folding efficiency and/or stability of AmyK38 prior to its release into the growth medium; (ii) indirect stabilization of AmyK38 through an increase in the net negative charge of the cell wall by not only the loss of protons, but also from the loss of D-alanine in the cell wall. (iii) reduced activities of the membrane-bound serine proteases HtrA and HtrB; and (iv) possible secondary effects of gene clusters activated or inactivated by increased external pH. These four possibilities cannot be discriminated by our present data, although the experiments using dltB mutants suggest that the loss of D-alanine esters due to an up-shift of external pH contributes to increased AmyK38 production. It should be mentioned that the alkaline α-amylase AmyK38 might fold effectively at alkaline external pH, which might increase the folding rate of AmyK38 as it emerges from the translocon, although experimental examination of this possibility is necessary.
Although it is common knowledge that strict pH control in fermentations is critical for optimal enzyme yields, our results demonstrate for the first time that RocG is an important factor influencing enzyme production by B. subtilis through its role in preventing acidification of the growth medium. Higher external pH enables more efficient secretion of the alkaline α-amylase AmyK38, likely due to the reduced accumulation of unfolded AmyK38 at the membrane-cell wall interface, and thus lowering the secretion stress. As alkaline α-amylases would be expected to fold more effectively at alkaline pH, we will verify our findings using other non-alkaliphilic α-amylases, such as AmyL and AmyQ, in future experiments. In addition, our results suggested that the loss of D-alanine esters in high external pH conditions additionally contributes to increased AmyK38 production. Importantly, under controlled pH conditions, reduced-genome strain MGB874 was found to be a beneficial host for the production of AmyK38 and yielded the highest levels of AmyK38 reported to date. For further improvement of AmyK38 production, we are presently attempting to generate an alkaline-tolerant mutant to reduce the remaining secretion stress response in B. subtilis.
Bacterial strains, plasmids, and growth media
Bacterial strains and plasmids used or constructed in this study
Strain or plasmid
Source or reference
MGB874 cat-rocDEF-rocR was inserted at the Δ(pdp-rocR) locus
MGB874 cat -rocR was inserted at the Δ(pdp-rocR) locus
MGB874 ΔaprE::Pspac-rocG spec (pAPNC213-rocG)
168 ΔamyE::PhtrB-lacZ cat (pDN110)
MGB874 ΔamyE::PhtrB-lacZ cat (pDN110)
MGB874 ΔaprE::Pspac-rocG spec ΔamyE::PhtrB-lacZ cat (pDN110)
supE44 Δ(mcrC-mrr) recA13 ara-14 proA2 lacY1 galK2 rpsL20 xyl-5 mtl-1 leuB6 thi-1
Shuttle vector for E. coli and B. subtilis
pHY300PLK carrying the gene for AmyK38 from Bacillus sp. strain KSM-K38 fused to the promoter, SD, and leader peptide sequences of egl-237, containing amp and tet
The integration vector containing Pspac promoter into the aprE locus by double crossover using spec
pAPNC213 containing the SD sequence and coding region of rocG (−25 to 1275, 1325 bp)
Integration vector for introduction of single-copy transcriptional fusions to lacZ by double crossover at the amyE locus (cat)
Construction of B. subtilis mutant strains
Primers used for the construction of B. subtilis mutants and plasmids are listed in (Additional file 3: Table S1). DNA manipulation techniques were as described previously . B. subtilis strain 874DEFRΔrocABC, in which the rocABC operon was substituted with the Sp-resistance gene (spec), was constructed from strain 874DEFR as follows. The spec gene was first amplified from pDG1727  using primers Spf and Spr. The approximately 1.0-kb flanking sequences located upstream (UProcABC) and downstream (DNrocABC) of the rocABC operon were then amplified by PCR from the strain 874DEFR genome using the primer pairs rocABCFW and rocABC/SpR, and rocABC/SpF and rocABCRV, respectively. The UProcABC and DNrocABC fragments overlapped with spec by 20 bp at the downstream and upstream ends, respectively. The three PCR fragments were then ligated in the order UProcABC-spec-DNrocABC by gene splicing using overlap extension PCR (SOE-PCR)  and the primers rocABCFW2 and rocABCRV2. The resulting 3.2-kb PCR product was used for the transformation of strain MGB874, and a positive Sp-resistant transformant was selected and designated as strain 874DEFRΔrocABC. Deletion of the rocABC operon was confirmed by PCR using primers rocABCFW and rocABCRV. A similar approach was used for the construction of mutant strains MGB625Δpdp-rocD, 168ΔcssRS, 874ΔcssRS, 168ΔdltB, and 874ΔdltB using the primers listed in (Additional file 3: Table S1). A 0.9-kb Cm-resistance gene (cat) fragment and 0.8-kb Nm-resistance gene (neo) fragment were PCR amplified from plasmids pC194  and pUB110 , respectively.
B. subtilis strain 874rocR was constructed using a similar approach to that used for the construction of strain 874DEFR . Briefly, strain MGB874 was transformed with chromosomal DNA from strain MGB625Δpdp-rocD, which only contains the rocR cat gene in the pdp rocR region of strain MGB625. As a result of the transformation, the rocR and cat fragment were reintroduced into the Δpdp rocR region in strain MGB874.
B. subtilis strain R-726, in which the rocG gene was expressed under control of the IPTG-inducible Pspac promoter from pAPNC213, was constructed as follows. A rocG gene fragment containing the ribosome-binding site of rocG was amplified and then cloned into the SalI/SacI sites of pAPNC213 . The resulting plasmid, named pAPNC213-rocG, was transformed into strain MGB874 to integrate the rocG gene into the aprE site by homologous recombination. A Sp-resistant transformant was selected and designated as strain R-726.
A transcriptional htrB lacZ fusion gene was generated by modification of plasmid pDL2 . First, plasmid pDN110 was constructed by cloning a 263-bp PCR-generated fragment (synthesized with primers YVTAPF and YVTAPR) using the procedure described by Noone et al . Strains R-1645, R-1646, and R-1926 were generated from strains 168, MGB874, and R-726, respectively, by the introduction of plasmid pDN110 and selection of Cm-resistant transformants.
Construction of expression vectors for the evaluation of exogenous enzyme production
Plasmid pHYK38 was used for the expression of alkaline α-amylase AmyK38 from Bacillus sp. strain KSM-K38  and was constructed as follows. A 1.5-kb DNA fragment coding for the mature form of AmyK38 was PCR amplified using genomic DNA extracted from Bacillus sp. KSM-K38 strain as template and primers K38matu-F2 (ALAA) and K38matu-R (XbaI) (Additional file 3: Table S1). In addition, a 0.6-kb DNA fragment including the promoter, Shine-Dalgarno (SD) sequence, and coding region for the signal sequence of the alkaline cellulase Egl-237 was PCR amplified using Bacillus sp. KSM-S237 genome as template and primers S237ppp-F2 (BamHI) and S237ppp-R2 (ALAA) (Additional file 3: Table S1). The amplified 1.5-kb and 0.6-kb fragments were fused together by SOE-PCR with primers S237ppp-F2 (BamHI) and SP64K38-R (XbaI) (Additional file 3: Table S1) to generate a 2.1-kb DNA fragment containing the AmyK38 gene downstream of the promoter, SD sequence, and coding region of the egl-237 signal sequence. The 2.1-kb DNA fragment was then inserted into the BamHI-XbaI cleavage site of the shuttle vector pHY300PLK (Takara Bio, Inc.) .
Viable cell counts
The detection of viable bacteria was performed by cultivation on agar plates and enumeration of colony-forming units (CFU). For each bacterial sample, a dilution series of cell suspensions was plated on LB agar plates, incubated overnight at 37°C, and colonies formed on the agar plates were then enumerated.
Culture method for assessment of AmyK38 production
B. subtilis mutants were transformed with pHYK38 by the protoplast transformation method, as previously described . To assess AmyK38 production levels, cells were pre-cultured in LB medium supplemented with 15 μg ml-1 Tet at 30°C for 15 h with shaking at 120 rpm, and 600 μl of the pre-culture broth was then inoculated into 30 ml 2xL-Mal medium in a 500-ml Sakaguchi flask. After further cultivation at 30°C with shaking at 120 rpm, cells were removed by centrifugation at 9,000 x g for 10 min, and α-amylase activity in the culture supernatant was then determined, as described below.
Amylase activity assay
α-amylase activity in culture supernatants was measured using a Liquitec Amy EPS kit (Roche Diagnostics), which uses 4,6-ethylidene-4-nitrophenyl-α-D-maltoheptaoside as a substrate . Culture broth supernatants were diluted 676-fold with 125 mM glycine-NaOH buffer (pH 10.0). As the pH of diluted samples was 10.0 after dilution, it appears that the pH of the growth medium did not influence the measured α-amylase activity. After sample preparation, 100 μl of R1-R2 mixture (R1 [coupling enzyme]: R2 [amylase substrate] = 5 : 1 [vol] was mixed with 50 μl of diluted sample solution, and the amount of p-nitrophenol released during incubation at 30°C was quantitatively determined by the change in absorbance at 405 nm (A405). The amount of enzyme required for the release of 1 μmol p-nitrophenol per minute was defined as 1 unit (U).
Purification of AmyK38
For the purification of AmyK38, B. subtilis strain 168 harboring pHYK38 was cultivated in 2xL-Mal medium at 30°C for 72 h. The purification procedure was performed as described by Hagihara et al. , with only minor modifications. Briefly, the centrifuged supernatant of the culture broth was loaded onto a Biogel P-6 DG desalting column (Bio-Rad Laboratories) equilibrated with 10 mM Tris–HCl buffer (pH 7.0). The eluate was collected as a single fraction and subjected to further purification by chromatography using a DEAE-Toyopearl 650 M column (Tosoh, Tokyo, Japan) and the identical protocol. Purified protein was quantified by a modified method of Lowry et al.  using the DC Protein Assay kit (Bio-Rad) and bovine serum albumin as the standard. The specific activity of purified AmyK38 towards 4,6-ethylidene-4-nitrophenyl-α-D-maltoheptaoside, as measured using a Liquitec Amy EPS kit (Roche Diagnostics) was 22,800 U mg protein-1.
Rabbit polyclonal antibodies against purified AmyK38 protein were prepared by Operon Biotechnology Co. (Tokyo, Japan).
Culture samples were harvested, and cells were then separated from the culture medium by centrifugation. The resulting supernatants were diluted 40-fold with 10 mM Tris–HCl (pH 7.0) containing Complete Mini Protease Inhibitor Cocktail Mixture (Roche Applied Science). Cells were washed twice with fresh 2xL-Mal medium, and re-suspended to an OD600 of 3.0 in 10 mM Tris–HCl (pH 7.0) containing the cocktail mixture. After adding 3x SDS-PAGE Loading Buffer (BioVision), the samples were incubated at 95°C for 1 min. For Western blotting analysis, the samples were subjected to sodium dodecyl sulfate polyacrylamide gel electrophoresis (SDS-PAGE) using 10% polyacrylamide gels (Ready Gels; Bio-Rad Laboratories) and 1x Tris-glycine-SDS running buffer (Bio-Rad Laboratories). The separated proteins were transferred to a PVDF membrane using a semi-dry transfer apparatus (Bio-Rad Laboratories) and then probed with primary antibodies against AmyK38 (1:2500) and visualized with a Western Breeze Colorimetric kit (Invitrogen) according to the manufacturer’s instructions. MagicMark XP Western Protein Standard (Invitrogen) was used as a protein standard.
Preparation of culture supernatants for assessment of AmyK38 stability
B. subtilis cells harboring pHYK38 were grown for 48 h in 30 ml 2xL-Mal medium, and cells were then removed by centrifugation at 9,000 x g for 30 min at 4°C. The obtained supernatants were filtered through a 0.22-μm pore-size MF microfilter (Millipore) to ensure the complete removal of cellular material. The cell-free supernatants were incubated at 30°C, and samples were removed at various intervals for the determination of α-amylase activity and Western blotting analysis.
The β-galactosidase assay was performed according to the method described by Hyyryläinen et al. . Briefly, cells were collected from 50 μl samples by centrifugation at 12,000 x g for 2 min at 4°C and were then washed once in 0.5 ml ice-cold 25 mM Tris–HCl (pH 7.4). After centrifugation at 12,000 x g for 2 min at 4°C, the pellet was first re-suspended in 0.64 ml Z buffer (60 mM Na2HPO4-H2O, 40 mM NaH2PO4-H2O, 10 mM KCl, and 1 mM MgSO4-7H2O) supplemented with 2 mM dithiothreitol (DTT) and then mixed with 0.16 ml lysozyme solution (2.5 mg/ml). After a 10-min incubation at 37°C, the sample was mixed with 8 μl 10% (v/v) Triton-X 100 and then stored at −30°C until assayed. The assay was initiated by the addition of 0.2 ml ο-nitrophenyl-β-D-galactoside (ONPG; 4 mg dissolved in Z buffer) to the pre-warmed sample, followed by incubation of the resulting mixture at 30°C. The reaction was terminated once the mixture turned yellow by adding 0.4 ml 1 M Na2CO3, and the total incubation time was recorded. β-galactosidase-specific activities are reported in units (U) and were calculated using the formula: 1000 x A420/reaction time (min) x OD600 of culture.
Measurement of ammonia concentration
The concentration of ammonia in culture supernatants was determined by enzymatic analysis according to the F-Kit UV method (Boehringer GmbH).
Measurement of sugar concentration
Sugars were analyzed by the phenol-sulfuric acid method . Briefly, 0.2-ml aliquots of diluted culture supernatants were mixed with an equal volume of 5% (w/v) phenol. One milliliter of concentrated sulfuric acid was then added and the mixture was mixed well. Following incubation at room temperature for 30 min, the absorbance of each sample was measured at 492 nm (A492). The concentration of sugars was calculated with a standard curve using known concentrations of glucose.
Quantitative real-time PCR
Total RNA was extracted from B. subtilis cells, as described previously , and reverse transcribed to cDNA using an AffinityScript QPCR cDNA Synthesis kit (Stratagene). As negative controls, all RNA samples were subjected to the identical reaction conditions without reverse transcriptase. qRT-PCR amplification, detection, and analysis were performed with the Mx3005P Real-time PCR System (Stratagene) and Brilliant II Fast SYBR Green QPCR Master Mix (Stratagene). The primer sequences used for qRT-PCR were designed using Primer 3 (version 0.4.0)  and are listed in (Additional file 4: Table S2). The source code of Primer 3 is available at http://frodo.wi.mit.edu/primer3/.
qRT-PCR was performed in 25-μl reaction mixtures consisting of 1xSYBR Green master mix, 0.4 μM of each forward and reverse primer, 3.2 μM reference dye, and 10 μl template. The PCR conditions were 95°C for 2 min, followed by 40 cycles of 95°C for 5 s and 60°C for 20 s. Amplified products were confirmed by dissociation curve analysis. To estimate the quantity of initial template DNA in samples, serial qRT-PCRs were performed by amplifying inserted target DNA in pUC118 (Takara Bio, Inc.) with specific primers. For each target gene, a standard curve was generated using the log of the quantity of initial template DNA plotted against the threshold cycle (Ct) values for the standard wells. The generated standard curves were used to convert the Ct values of each amplified gene in the cDNA preparations to copy numbers of cDNA molecules. The estimated copy number was normalized to the value for 16 S rRNA, as previously described .
Control secretion stress Regulator and Sensor
Generally Regarded as Safe
Quantitative real-time PCR
Sodium dodecyl sulfate polyacrylamide gel electrophoresis
We thank Junichi Sekiguchi (Shinshu University), Kouji Nakamura (University of Tsukuba), Shigehiko Kanaya, Shu Ishikawa (Nara Institute of Science and Technology), Fujio Kawamura (University of Rikkyo), and Yasutaro Fujita (Fukuyama University) for valuable discussions. We also thank Yoshiharu Kimura and Yoshinori Takema (Kao Corp.) for valuable advice. This study was performed in collaboration with Takuya Morimoto (Kao Corp.), Shengao Liu (Kao Corp.), Takeko Kodama (Kao Corp.), and Hiroshi Kakeshita (Kao Corp.).
This research was conducted as part of the Project for the Development of a Technological Infrastructure for Industrial Bioprocesses through R&D on New Industrial Science and Technology Frontiers of the Ministry of Economy, Trade, and Industry (METI), Japan, and was supported by the New Energy and Industrial Technology Development Organization (NEDO), Japan.
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