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Journal of Bacteriology, August 2001, p. 4905-4909, Vol. 183, No. 16
0021-9193/01/$04.00+0   DOI: 10.1128/JB.183.16.4905-4909.2001
Copyright © 2001, American Society for Microbiology. All rights reserved.

Control of a Family of Phosphatase Regulatory Genes (phr) by the Alternate Sigma Factor Sigma-H of Bacillus subtilis

Ryan S. McQuade, Natalia Comella, and Alan D. Grossman*

Department of Biology, Massachusetts Institute of Technology, Cambridge, Massachusetts 02139

Received 16 March 2001/Accepted 21 May 2001


    ABSTRACT
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A family of 11 phosphatases can help to modulate the activity of response regulator proteins in Bacillus subtilis. Downstream of seven of the rap (phosphatase) genes are phr genes, encoding secreted peptides that function as phosphatase regulators. By using fusions to lacZ and primer extension analysis, we found that six of the seven phr genes are controlled by the alternate sigma factor sigma-H. These results expand the potential of sigma-H to contribute to the output of several response regulators by controlling expression of inhibitors of phosphatases.


    TEXT
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A family of phosphatases and cognate regulators (Fig. 1) modulate the output of two-component signal transduction systems in Bacillus subtilis (19, 31, 34). Two-component systems generally consist of a histidine protein kinase that autophosphorylates on a histidine residue and a response regulator, often a transcription factor, whose activity is controlled by phosphorylation of an aspartate residue (10, 11). The response regulator obtains phosphate from its cognate kinase. Many cellular processes are controlled by two-component systems: the B. subtilis genome encodes 37 histidine kinases and 34 response regulators (5, 16).


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  		FIG. 1.   The family of rap phosphatases and phr peptide regulators. Putative transcriptional start sites, as determined by mapping 5' ends by primer extension analysis, are indicated by arrows. To analyze expression, DNA fragments (denoted by solid lines underneath the genes) were cloned upstream of lacZ and integrated into the chromosome at amyE. The fragments were amplified by PCR with Vent polymerase and primers with restriction sites (EcoRI and BamHI) at the ends. These fragments were subcloned between the EcoRI and BamHI sites of pKS2 (23). The resulting plasmids were linearized and transformed into wild-type B. subtilis, selecting for Neor transformants. Transformants were screened for an amylase-deficient phenotype to confirm the plasmid had integrated into the chromosome at the amyE locus. For each phr gene, the fragment end points are indicated relative to the translation start site: phrA, 530 bp upstream, 30 bp downstream; phrE, 275 bp upstream, 73 bp downstream; phrF, 749 bp upstream, 62 bp downstream; phrG, 745 bp upstream, 30 bp downstream; phrI, 465 bp upstream, 37 bp downstream; phrK, 583 bp upstream, 22 bp downstream.

The phosphorylation state of many response regulators is negatively regulated by phosphatases. B. subtilis has a family of 11 genes encoding phosphatases (or putative phosphatases) that are homologous to each other (16, 29, 34). Several of these response regulator aspartyl phosphate phosphatases (Rap phosphatases) have been characterized. RapA and RapB (and to a lesser extent RapE) negatively regulate the initiation of sporulation (14, 25, 30, 31). They do so by dephosphorylating the response regulator protein Spo0F, which is part of the phosphorelay (1) that is required to activate the sporulation transcription factor Spo0A in response to multiple signals, including starvation (6, 12, 31).

The activities of RapA, RapB, and RapE are negatively regulated by specific pentapeptides. RapA and RapE are inhibited by the pentapeptides produced from precursors encoded by phrA and phrE, the genes downstream from rapA and rapE, respectively (14, 28, 33). RapB is inhibited by the pentapeptide that is produced from the precursor encoded by phrC, the gene downstream from rapC (28). These inhibitory peptides are exported, and at least some of them accumulate in culture supernatant. They are then imported by the oligopeptide permease (Opp [also known as Spo0K]) (20, 32, 38). In this way, the peptides can be indicators of population density (17, 18, 20, 33, 40), as well as the intracellular conditions necessary for their production (18, 28, 29).

The pentapeptide produced from the phrC gene product, called CSF (competence and sporulation-stimulating factor), was initially purified from culture supernatant as an activity that stimulates expression of genes activated by the transcription factor ComA (40, 41). comA encodes a response regulator required for the development of genetic competence (26, 45) and the general quorum response (17, 19). ComA is active in the phosphorylated form and obtains phosphate from the histidine kinase ComP (15, 36, 37, 46). RapC inhibits expression of genes activated by ComA~P, most likely by dephosphorylating ComA~P (40). Expression of genes activated by ComA~P is increased by two different extracellular peptides, the ComX pheromone, which activates the kinase ComP (23, 36, 41), and CSF, which appears to inhibit the phosphatase RapC (41). In this way, two different extracellular signaling molecules contribute to activate a general quorum response controlled by ComA.

Transcription of phrC is controlled by two promoters: P1, which is upstream of rapC and directs transcription of rapC and phrC (18); and P2, which is internal to rapC and directs transcription of phrC (2, 18). Transcription from P2 is controlled by the alternate sigma factor sigma-H (the product of sigH [also known as spo0H]) and increases during entry into stationary phase (2, 18). phrE is also dependent on sigma-H for maximal expression (14).

A phr gene, encoding a putative or bona fide secreted peptide that functions as a phosphatase regulator, is found downstream from 7 of the 11 rap genes (Fig. 1). We have found that, with the exception of phrA, all of the phr genes have sigma-H promoters upstream of the gene and internal to the cognate rap gene. These findings indicate that the alternate sigma factor sigma-H controls production of a family of phosphatase regulators and that synthesis of these regulators is controlled by the nutritional conditions that modulate sigma-H.

Expression of phr-lacZ fusions. A search of the B. subtilis genome found putative sigma-H promoters upstream of each phr gene, except phrA (19). To measure expression from the potential promoters upstream of the phr genes and to test the dependence on sigma-H, we constructed transcriptional fusions of the regions upstream of the phr genes to lacZ (Fig. 1 and Table 1). We amplified the putative promoter regions by PCR and cloned the fragments upstream from lacZ, and the resulting fusions were integrated into the chromosome at a heterologous site (amyE). We measured beta -galactosidase specific activity for each fusion during growth and after entry into stationary phase in nutrient broth sporulation medium (Fig. 2) and defined minimal medium (data not shown) at 37°C. The patterns of expression were similar in both media. All of the fusions had an initially low level of expression that increased at or shortly before the transition to stationary phase (T0). The peak of beta -galactosidase specific activity was between 1 and 3 h after the end of exponential growth. No expression was observed from a fusion made to the region upstream of phrA (data not shown), indicating that under the conditions tested, there is not a functional promoter in this region.

                              
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  		TABLE 1.   B. subtilis strains used in this study



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  		FIG. 2.   Expression of the phr-lacZ transcriptional fusions. beta -Galactosidase specific activity was assayed as described previously (13, 24). The time indicated is relative to the transition to stationary phase (T0). (A) phrE-lacZ. (B) phrF-lacZ. (C) phrG-lacZ. (D) phrI-lacZ. (E) phrK-lacZ. Solid circles, wild type; open triangles, sigH; solid triangles, spo0A; solid squares, abrB; open squares, spo0A abrB. Strains are indicated in Table 1.

A sigH null mutation reduced the maximal level of expression to less than 1% of that of the wild type for all fusions, except phrE and phrI (Fig. 2). The phrE- and phrI-lacZ fusions retained a significant level of expression in a sigH null mutant (Fig. 2A and D), presumably due to transcription from the sigma-A promoters described below. The pattern of expression seen for the phrE-lacZ fusion is consistent with that described previously (14).

Spo0A and AbrB affect expression of many sigma-H-regulated promoters (6, 8, 35, 42, 47, 48). In a spo0A null mutant, transcription of phrCP2 is decreased ~5-fold during stationary phase. This effect is relieved by a null mutation in abrB (2, 18). Similar effects were observed with the other phr-lacZ fusions (Fig. 2). In all cases, a spo0A null mutation caused a decrease in activity compared to that of the wild type, and this effect was relieved by a null mutation in abrB.

The expression of the phrE-lacZ and phrI-lacZ fusions was significantly higher in the abrB null mutant than in the wild type (Fig. 2A and D). There are sequences in these promoter regions that resemble known AbrB binding sites (42), and we suspect that AbrB acts directly to repress expression from phrEP1 and/or -P2 and phrIP1.

Primer extension mapping of phr promoters. The lacZ fusions confirmed the existence of promoters upstream of the phr genes. To determine if the location of the promoters correlated with the sequences resembling sigma-H-dependent promoters, we used primer extension to map precisely the 5' ends of transcripts of phrE, phrF, phrG, phrI, and phrK (Fig. 3). Cells were grown in sporulation medium (39) at 37°C, and RNA was prepared from cells 2 to 3 h after the end of exponential growth. Primer extension was performed essentially as described previously (43). The major primer extension products for all of the genes correlated to start sites downstream from the putative sigma-H promoters (Fig. 3). Furthermore, these products were not observed in a sigH null mutant (Fig. 3) (data not shown). phrE and phrI also had primer extension products that were not dependent on sigma-H (Fig. 3A and D), consistent with the pattern of expression of the phrE-lacZ and phrI-lacZ fusions (described above).


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  		FIG. 3.   Primer extension mapping of the 5' ends of phr mRNA and sequences of the promoter regions. (A to F) RNA for primer extension was prepared by the Qiagen RNeasy protocol. Approximately 50 µg of RNA was used per primer extension reaction. Each primer extension reaction is shown alongside a sequencing ladder (lanes labeled GATC) produced with the same end-labeled primer. RNA was prepared from wild-type (wt) cells (IRN238 or RSM128) and a sigH mutant (lane H [IRN243 or RSM135]). (A) phrE, primer phrE4 (5'-CCAATTAAAACGGCGGATAAACTGA-3'). (B) phrF, primer phrF5 (5'-GAGCCAGACAAGAGAGTAATAGTTTAGA-3'). (C) phrG, primer RM36 (5'-CTTACACTGTCATACTCTTTCTCGGAC-3'). (D) phrIP1, primer phrIPEU (5'-CGTCTTGCTTCAATACTCATACG-3'). (E) phrIP2, primer phrIPE (5'-CTATGCCCCTACCCGATCTGCAGC-3'). (F) phrK, primer RM38 (5'-GCTCGTTGCTTCTTCAAAAGCACC-3'). (G) Sigma-H promoters identified by primer extension analysis. Promoters were aligned by the -10 region with spaces added to align the -35 regions. Residues with identity to the sigma-H consensus sequence are indicated in boldface. The transcription start sites (+1) as determined by primer extension are indicated by boldface, lowercase letters. The sigma-A consensus site in phrEP1-2 is underlined.

phrE transcripts had three detectable 5' ends (Fig. 3A). The level of each was reduced in a sigH null mutant, with the two downstream ends reduced below the limit of detection. The most upstream end (P1) corresponds to a potential sigma-A promoter, and the two downstream ends (P2 and P3) correspond to potential sigma-H promoters. We suspect that the effect of the sigH null mutation on P1 is due to the effects of sigH on expression of spo0A, which is required for full expression of phrE (Fig. 2A) (14).

phrI had two apparent 5' ends corresponding to promoters of two different sigma factors (Fig. 3D to E). The upstream product was independent of sigma-H and corresponds to the start site for a potential sigma-A promoter (P1). The downstream product was not observed in a sigH null mutant and matches the start site of the sigma-H promoter (P2) predicted by sequence analysis.

Sigma-H and regulation of response regulators. The characterized Phr peptides act as extracellular regulators of gene expression by inhibiting Rap phosphatases that act on response regulators (14, 20, 28, 40). The remaining phr genes are predicted to encode similar extracellular peptides that regulate the activity of other Rap phosphatases (34). The finding that all of the phr genes (except phrA) are transcribed by RNA polymerase holoenzyme containing sigma-H implies that many cellular processes and response regulators are regulated indirectly by sigma-H.

Sigma-H is regulated by many diverse signals, and this regulation occurs at the transcriptional and posttranslational levels. The activity of sigma-H is regulated by growth phase (9, 47), pH (3), members of the Clp protease family (21, 22, 27), and perhaps the stringent response (4). As cells experience conditions that increase activity of sigma-H, the amount of phr transcription relative to its upstream rap will increase. This will enhance the regulation (inhibition) of the Rap phosphatases by their respective Phr peptides.

The effects of sigma-H on control of expression of the phr genes most likely contribute to the effects of cell culture density on sporulation. Sporulation is more efficient at high than low cell densities (7, 12, 20, 44), due to the accumulation of signaling peptides in culture supernatant (7, 20). sigH mutants are defective in production of at least some of the signaling peptides (7, 20). We suspect that several other cellular responses are modulated by population density and that sigma-H contributes to these via its role in expression of the phr genes.


    ACKNOWLEDGMENTS

We thank members of the laboratory for useful discussions and especially R. A. Britton and E. Küster-Schöck for comments on the manuscript.

R.S.M. and N.C. were supported in part by National Institutes of Health (NIH) predoctoral training grants, and this work was supported in part by Public Health Service grant GM50895 from the NIH.


    FOOTNOTES

* Corresponding author. Mailing address: Department of Biology, Building 68-530, Massachusetts Institute of Technology, Cambridge, MA 02139. Phone: (617) 253-1515. Fax: (617) 253-2643. E-mail: adg{at}mit.edu.


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Journal of Bacteriology, August 2001, p. 4905-4909, Vol. 183, No. 16
0021-9193/01/$04.00+0   DOI: 10.1128/JB.183.16.4905-4909.2001
Copyright © 2001, American Society for Microbiology. All rights reserved.


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