The medical importance of many different secondary metabolites has resulted in the study of gene expression in numerous species of the evolutionarily deep genus Streptomyces, as for any particular secondary metabolite increased knowledge about its regulation expands the scope for the rationale design of approaches to improve yield and fermentation performance, at least in principle. Consequently, there is interest in determining to what extent regulators of secondary metabolism identified for one species have homologues with a role in the regulation of secondary metabolites for others. Here we have shown that the production in S. griseus of AtrAc, an activator of transcription of the CSR of the actinorhodin biosynthetic genes in S. coelicolor, causes a reduction in the biosynthesis of streptomycin (Fig. 2) and in the transcription of the corresponding CSR strR (Fig. 3). These results indicate that the atrA homologue in S. griseus, revealed here by Southern blot analysis (Fig. 1), merits further investigation as a potential regulator of streptomycin production.
The advantages of using the approach we used here to determine the extent to which a regulator of secondary metabolism has homologues that also have a role in the regulation of secondary metabolites in other species are that it requires no prior knowledge of the genome sequences of the species being screened and it is relatively straightforward to perform. Most Streptomyces species can readily receive plasmids by conjugation and have an integration site for the expression constructs used here (Combes et al. 2002). We are in the process of determining the effects producing AtrAc has on the production of known secondary metabolites by other species. At this stage we can report that while it stimulated the production of actinorhodin in S. lividans, a close relative, no effects were detected on the production of oxytetracycline or rimocidin by strains of S. rimosus (data not shown). The latter is not unexpected as our previous characterisation of atrAc revealed that it has specificity with regard to the biosynthetic genes it influences. Although disruption of the atrA gene in S. coelicolor reduced the production of actinorhodin, it had no detectable effect on the production of undecylprodigiosin or the calcium dependent antibiotic (Uguru et al. 2005).
We do not, however, conclude from our results that the S. griseus homologue of AtrA likely functions as a repressor of strR transcription. During the time S. coelicolor and S. griseus last shared a common ancestor, which has been estimated to be about 200 million years ago (Embley and Stackebrandt 1994), it is likely that the ancestral AtrA and its targets have coevolved (i.e. each have adapted to changes in the other) within both lineages. Therefore, even though a homologue may be able in a heterologous host to bind sites used by the native activator, this may not be sufficient for the former to stimulate transcription as it may be unable to make necessary contacts with RNA polymerase (for review, see Lloyd et al. 2001). Moreover, the co-expression of such a homologue may antagonize activation by the native activator as a result of competition for DNA binding. Thus, the finding that the expression of S. coelicolor AtrA reduces strR transcription in S. griseus by a DNA binding-dependent mechanism does not exclude the possibility that the native AtrAg homologue functions as an activator of strR transcription. Indeed, deletion analysis has revealed that a region containing a site to which AtrAc binds in vitro is required for maximum transcription of strR by an A-factor-independent mechanism (Vujaklija et al. 1991). Although, in comparison to identifying and knocking out the genes of homologues, the approach we used does not by itself provide a clear indication of the precise function of homologues, it nonetheless has value as a simple screen to investigate whether or not they have a role in regulating the production of a particular secondary metabolite.
Interestingly, the effect on the transcription of strR resulting from the expression of atrAc did not appear to be mediated via a change in the transcription of adpA, the only previously characterised regulator of strR (Fig. 3). In support of the latter point, the expression of atrAc had no discernible effect on S. griseus sporulation (data not shown), which is also under adpA control (for review, see Ohnishi et al. 2005; Horinouchi 2002). From the above results we conclude that, as implicit in the data of Vujaklija et al. (1993), the A-factor-ArpA-AdpA-StrR regulatory cascade represents only part of the full complexity of regulation of streptomycin biosynthesis in S. griseus. That a factor(s) in addition to AdpA regulates transcription from the strR promoter is not unusual, at least from the study of E. coli where it is rare for a promoter to be regulated in response to a single environmental or physiological signal (reviewed in Browning and Busby 2004). This conclusion stands irrespective of the precise role that transpires for the S. griseus homologue of AtrA.
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Fig. 1 The integration of plasmids in exconjugants of S. griseus. (A) The integration of a single copy of each plasmid was confirmed by Southern blot analysis of total DNA digested with BamHI and probed with a DIG-labelled segment of S. coelicolor atrA. The numbers at the top of the panel identify individual isolates of each of the strains. Lane M contains DIG-labelled DNA molecular weight marker II (λ/HindIII, Roche). (B) Integrated of plasmids at the attB site was confirmed by PCR using a primer that bound within this attachment site and another that bound within the backbone of pSET152. The desired integration produces a PCR product of 1.6 kbp. Lane M contains DNA size markers (1-kb DNA ladder, New England BioLabs), whereas lane C corresponds to strain ATCC12475, which served as a negative control. Numbers down the left of each panel indicate the sizes of specific DNA markers (kbp)
Fig. 2 The effect on streptomycin production of expressing S. coelicolor atrA in S. griseus. Multiple isolates of each strain were assayed in triplicate. Each point in the scatterplot represents the mean area of the zones of growth inhibition around a particular isolate. For each strain, a cross and bar indicates the mean and standard deviation, respectively, of the values obtained for different isolates. The arrows indicate the values of isolates that were chosen for further analysis (Fig. 3); these were BH646 #1 and BH152 #1. The insets show the actual zones of inhibition observed for these particular isolates; BH646 #1 on the right and BH152 #1 on the left
Fig. 3 The effects on transcription of strR, its regulon and adpA. (A) The relative abundance of the strR transcript in mycelial patches of strains BH646 #1 and BH152 #1 grown on YMPD agar plates for 2 and 3 d was determined using quantitative, real-time PCR analysis of reverse-transcribed RNA samples. The values were normalised using values obtained for hrdB mRNA. The error bars are derived from three estimates of the abundance of strR mRNA in each sample (see Experimental procedures). (B) The levels of the strB1, strD, hrdB and adpA transcripts in 2 days samples of BH646 #1 and BH152 #1 were analysed semi-quantitatively using end-point PCR analysis of the same reverse-transcribed RNA samples used in panel A
|(1)||Faculty of Biological Sciences, University of Leeds, Leeds, LS8 2BH, UK|
|(2)||Institute of Medicinal Biotechnology, Chinese Academy of Medical Sciences, Beijing, 100050, China|
|(3)||Institute for Innovation and Development of Learning Process, Mahdiol University, Rama VI, Bangkok, 10400, Thailand|
|(4)||Institute for Pharmacy and Biomedical Sciences, University of Strathclyde, Glasgow, G1 1XW, UK|
In Streptomyces coelicolor, AtrA is an activator of transcription of the actinorhodin cluster-situated regulator gene actII-ORF4. In previous work, we showed that S. coelicolor AtrA binds in vitro to the promoter of S. griseus strR, the streptomycin cluster-situated regulator. We show here that S. griseus carries a single close homologue of atrA and that expression of S. coelicolor AtrA in S. griseus causes a DNA binding-dependent reduction in streptomycin production and in the mRNA levels of strR and genes of streptomycin biosynthesis. However, there is no effect on the level of the mRNA of adpA, which is the only transcription factor that has so far been characterised for strR. The adpA gene is directly regulated by ArpA, the receptor protein for the γ-butyrolactone signalling molecule A-factor. Therefore, to our knowledge, our results provide the first in vivo evidence that A-factor-ArpA-AdpA-StrR regulatory cascade represents only part of the full complexity of regulation of streptomycin biosynthesis in S. griseus. The potential biotechnological application of our findings is discussed.
Keywords Actinorhodin - Secondary metabolite production - Streptomyces gene regulation - S. coelicolor - S. griseus - Streptomycin
Biotechnology Letters. © Springer Science+Business Media B.V. 2006.10.1007/s10529-006-9216-2.
Mycelial bacteria of the genus Streptomyces and their relatives produce a plethora of secondary metabolites including antibiotics, antihelminthics and anti-tumour agents in clinical use. Their yield and timing of formation are exquisitely sensitive to growth conditions and have been associated with the accumulation of signalling molecules such as γ-butyrolactones, a family of microbial hormones (Horinouchi 2002; Chater and Horinouchi 2003). In virtually all cases that have been studied in detail, a change in the production of a secondary metabolite has been correlated with a change in the transcription of an activator gene situated with the corresponding biosynthetic genes as part of a cluster (for review, see Chater and Bibb 1997; Bibb 2005). To date, the only system for which there is a well authenticated, completely ungapped regulatory pathway from a signal to the production of a secondary metabolite is the regulation of streptomycin production in S. griseus by the γ-butyrolactone A-factor, whose accumulation may serve to communicate or coordinate the behaviour of individual cells (Ohnishi et al. 2005). A-factor produced by S. griseus binds to the receptor protein ArpA, which then has reduced affinity for DNA and thus is a less effective repressor of AdpA, which directly activates strR (Ohnishi et al. 1999), the activator situated in the streptomycin cluster, as well as several genes required for morphological differentiation (Ohnishi et al. 1999; Yamazaki et al. 2000, 2003a, b; Kato et al. 2002). It has been reported (Vujaklija et al. 1993) that as well as AdpA, other unidentified proteins bind upstream of strR; however, the role of the latter factors in mediating the response to A-factor or some other signal remains to be established.
The actinorhodin system in S. coelicolor has been studied in detail and numerous genes have been identified that affect the production of this secondary metabolite (Hopwood et al. 1995; Bibb 1996). Recently, we described the characterisation of AtrA, a transcription factor required for maximum transcription of actII-ORF4, the cluster-situated regulator (CSR) of the actinorhodin biosynthesis genes in S. coelicolor. Like many of the genes that regulate actinorhodin production, atrA does not have an orthologue in published models for the regulation of streptomycin production by S. griseus. As part of our previous study, we found that S. coelicolor AtrA can bind in vitro to the promoter of strR (Uguru et al. 2005). This finding raised the possibility that the regulation of streptomycin production, which serves as an important model, may involve a homologue of S. coelicolor AtrA. The results presented here show that S. griseus carries a single close homologue of atrA and that expression of S. coelicolor AtrA (AtrAc) in S. griseus can affect streptomycin production by a mechanism that is independent of change in the AdpA step of the A-factor cascade. The possible biotechnological implications of our findings are discussed.
Integrating plasmids pL646 and pL644, which constitutively express wild-type AtrA and an Arg 71 to Ala (R71A) mutant, respectively, were transferred by conjugation from Escherichia coli ET12567 (pUB307) (Flett et al. 1997) to S. griseus ATCC 12475 (Vallins and Baumberg 1985) using an established protocol (Kieser et al. 2000). These constructs were based on a pSET152-based integrating expression construct (Tilley 2003) that uses the constitutive ermE*p promoter (Schmitt-John and Engels 1992; Bibb et al. 1994) and the ribosome-binding site of the tuf1 gene (van Wezel et al. 2000). Exconjugants were selected with apramycin (50 μg ml−1) and the resulting strains were designated BH646, BH644 and BH152, respectively. Integration at the attB site in the S. griseus chromosome (Combes et al. 2002) was confirmed initially by a PCR assay using primers that hybridised to sites within attB (5′-CGG TGC GGG TGC CAG GGC) and the backbone of pSET152 (5′-TTC GGC GGC TTC AAG TTC GG), respectively.
Total DNA was prepared as described previously (Kieser et al. 2000) from mycelia grown in YMPD liquid medium (Ohnishi et al. 1999) and cut using BamHI. After agarose gel electrophoresis, the DNA was transferred to a Zeta-Probe GT blotting membrane (BioRad) using a capillary blotting stack (Maniatis et al. 1982), and fixed to the membrane using a UV Stratalinker (Stratagene). The digoxigenin (DIG)-labelled DNA probe for the atrA gene was generated using the PCR DIG Probe Synthesis Kit (Roche). The primers were AtraAF (5′-GGA TCC TCA GGA TTC TCA TTG GTC GTC) and AtraAR (5′-GGA TCC GTG GCT ATG ACC AGC AGC AC). The membrane was prehybridised at 55°C for at least 30 min using the DIG Easy Hyb hybridisation buffer (Roche), denatured DIG-labelled probe was added and incubated continued overnight at the same temperature. After hybridisation, the membrane was washed twice with low stringency buffer (2 × SSC, 0.1% w/v SDS) at room temperature and twice with high stringency buffer (0.1 × SSC, 0.1% w/v SDS) at 68°C. At this temperature, only genes that have 80–100% sequence identity with the probe are bound (DIG Application Guide for Filter Hybridization, Roche). For the detection of probe, the membrane was washed and blocked using the DIG Wash and Block Buffer Set (Roche), incubated with anti-DIG-alkaline phosphatase antibody (Roche), and then incubated with a chromogenic substrate for alkaline phosphatase, Nitro-Blue tetrazolium chloride/5-bromo-4-chloro-3′-indolyphosphate p-toluidine salt.
The bioassay of streptomycin essentially followed a method described previously (Horinouchi et al. 1984). The indicator was Bacillus subtilis 168 obtained from Dr. Keith Stephenson, University of Leeds. The specificity was checked by the parallel use of streptomycin-sensitive or -resistant E. coli. 245 × 245 mm2 bioassay dishes (Corning) containing 150 ml of Bennett’s medium in 2% (w/v) agar No. 1 (LAB M) were spotted at 3 cm intervals with 3 × 106 spores. The plates were incubated at 30°C for 2 days before being overlaid with 50 ml of Bennett’s soft agar containing 2.1 ml of a culture of the indicator at OD600 0.5, which had been grown in LB medium at 37°C. After another day of incubation at 30°C, the area of the ring of inhibition of indicator growth around each patch of S. griseus was measured. Standard conditions were used for the preparation and quantitation of spores (Kieser et al. 2000).
RNA was isolated, quantitated, and reverse transcribed as described previously (Uguru et al. 2005). The RNA was isolated from S. griseus mycelia scraped from cellophane (AA Packaging, UK) laid on the surface of YMPD agar plates. The level of the strR transcript in samples from mycelial patches of different age was analysed in real time as described previously (Uguru et al. 2005) using primers strR_FOR (5′-GAG CAA GTC CGT GAG AGG TC) and strR_REV (5′-GAG GGA AGC AAT GAT TCG AC). As before (Uguru et al. 2005), the values were normalised using the level of hrdB mRNA as a control. The PCR reaction conditions were 95°C for 7 min followed by 45 cycles of 95°C for 30 s, 56°C for 30 s, 72°C for 40 s. The temperature at which fluorescence was measured at the end of each cycle was 83°C. The relative levels of several transcripts in samples from mycelial patches of the same age were analysed semi-quantitatively using end-point analysis. The primers for the amplification of segments of hrdB (127 bp), strB1 (123 bp), strD (125 bp) and adpA (130 bp) mRNA were 5′-TGG TCG AGG TCA TCA ACA AG with 5′-TGG ACC TCG ATG ACC TTC TC, 5′-GAC GGG TTC CAC GAC TAC TG with 5′-CAG CAG GAG GTC CTT GTA G, 5′-GTC GCC GAG ATA CAT GAT GA with 5′-ATG GTT CGA GAT TCG GAC TG, and 5′-CGA TCT CTG CCT CCA CAT AG with 5′-CTC CGG TAA AGA CCT GTC CA, respectively. The size of each amplicon is provided in the parentheses. The PCR conditions for end-product analysis were standard PCR reactions using PCR reaction buffer Mix J (Epicenter) and 10% (v/v) DMSO (Sigma). The reactions were done in 0.2 ml thin-wall tubes (BIOplastics) using a standard PCR machine with a heated lid (MiniCycler, MJ Research) and the final products were analysed by gel electrophoresis in TBE-buffered 2% (w/v) agarose. The reactions were incubated at 95°C for 5 min followed by 40 cycles of 95°C for 30 s, 56°C for 30 s, and 72°C for 40 s.