Since high-value bacterial secondary metabolites, including antibiotics, are often naturally produced in only low amounts, their efficient biosynthesis typically requires the transfer of entire metabolic pathways into suitable bacterial hosts like Pseudomonas putida. Stable maintenance and sufficient expression of heterologous pathway-encoding genes in host microbes, however, still remain key challenges. In this study, the 21 kb prodigiosin gene cluster from Serratia marcescens was used as a reporter to identify genomic sites in P. putida KT2440 especially suitable for maintenance and expression of pathway genes. After generation of a strain library by random Tn5 transposon-based chromosomal integration of the cluster, 50 strains exhibited strong prodigiosin production. Remarkably, chromosomal integration sites were exclusively identified in the seven rRNA-encoding rrn operons of P. putida. We could further demonstrate that prodigiosin production was mainly dependent on (i) the individual rrn operon where the gene cluster was inserted as well as (ii) the distance between the rrn promoter and the inserted prodigiosin biosynthetic genes. In addition, the recombinant strains showed high stability upon subculturing for many generations. Consequently, our findings demonstrate the general applicability of rDNA loci as chromosomal integration sites for gene cluster expression and recombinant pathway implementation in P. putida KT2440.
Microbial natural products are an invaluable source of bioactive compounds such as antibiotics. Since these high-value metabolites are often naturally produced in only low amounts or the natural producers are not amenable to genetic engineering and bioprocess development, efficient biosynthesis of these compounds, enabling studies e.g. on their bioactivities or the underlying biocatalytic reactions, typically requires the transfer of entire metabolic pathways into heterologous expression hosts1.
The Gram-negative γ-proteobacterium Pseudomonas putida is especially suited for heterologous secondary metabolite biosynthesis, because its metabolism is supportive of various natural product pathways and conveys broad tolerance to compounds which are toxic to other bacteria2,3. Therefore, multiple tools including vector and promoter sets have been developed to enable functional gene expression in this host4,5,6. In addition, since the stable maintenance and strong expression of pathway-encoding gene clusters still represent major bottlenecks for effective production7, the chromosomal integration of target genes is gaining more and more interest8,9.
In our previous studies, we established the pathway transfer and expression (TREX) system, which allows the straightforward implementation of heterologous secondary metabolite pathways in different bacterial species. TREX employs the random chromosomal integration of a target gene cluster by Tn5-based transposition, followed by the concerted expression of all biosynthetic genes. This can be realized by use of T7 RNA polymerase-dependent promoters10 or an intrinsically strong chromosomal promoter like those driving expression of the ribosomal RNA-encoding genes of P. putida KT244011,12. Chromosomal insertion of foreign biosynthetic genes downstream of the latter may be especially favorable for the functional expression of a biosynthetic pathway because this locus possesses two specific characteristics: (i) In P. putida KT2440, the ribosomal RNA, i.e. 5S, 16S and 23S rRNA, is encoded in seven rRNA operons, also referred to as rrn operons or rDNA, across the bacterial chromosome13,14. Although rRNA generation is essential for maintaining cellular life, the insertion of genes in one rrn operon copy is not deleterious due to the gene redundancy11,15. (ii) At the same time, the promoters of rrn operons are commonly regarded as highly active16. This may be particularly relevant in the implementation of transcription levels required for the functional expression of large gene clusters since the likelihood of eventual (Rho mediated) RNA polymerase dissociation17 from the template increases with the transcript length. Together with mRNA degradation at the 3′ terminus18,19, this can cause low transcript levels of distal genes. A strong promoter may help to maintain sufficient transcript levels of genes at the end of the transcriptional unit, while the 3′ fusion of the mRNA with the highly stable rRNA could decrease the rate of degradation. Such chromosomal loci can thus be of particular relevance for the implementation of a heterologous biosynthetic pathway in P. putida, and can be identified e.g. by Tn5 transposition.
In the present study, we intended to further pursue this approach in order to identify additional chromosomal loci of P. putida suitable for the stable integration and strong expression of clustered biosynthetic genes by a native promoter. To this end, the 21 kb prodigiosin gene cluster (pig) from Serratia marcescens was used as a ‘reporter gene cluster’ because functional expression of all cluster genes in P. putida results in a red phenotype that can easily be screened for by visual inspection. To search for suitable genomic loci within the entire chromosome of P. putida KT2440, we created a pig strain library by applying genomic integration of the pathway genes via Tn5-based random transposition. Based on intense red coloration phenotypes, a set of 50 strains synthesizing the pigment was identified and analyzed with respect to individual chromosomal insertion loci and corresponding prodigiosin production titers. Remarkably, in all of the analyzed P. putida strains, the pig cluster was integrated in one of the seven rrn operons. Prodigiosin levels were strongly influenced by the specific rrn operon copy in which the biosynthetic genes were inserted and further modulated by the distance between the rrn promoter and inserted pig genes. This study therefore demonstrates the applicability of the P. putida rrn operons as particularly suitable gene cluster integration sites potentially allowing the identification and synthesis of new and valuable natural products in this versatile production host.
Generation of a P. putida TREX-pig strain library
In order to identify locations in the chromosome of P. putida KT2440 which allow the activation of a heterologous biosynthetic pathway – a process that includes the stable insertion and expression of multiple pathway genes – we employed transposon Tn5-based integration of the prodigiosin gene cluster (pig) from S. marcescens. Transposon Tn5 is a widely established tool for untargeted gene integration into the bacterial chromosome and permits an almost completely unbiased sampling of the chromosomal space20,21,22. The pig gene cluster is particularly suited as a ‘reporter gene cluster’ for the following reasons: (i) The pigA-N gene cluster comprises 14 genes spanning 21 kb and can thus be regarded as a representative of a multitude of mid-sized biosynthetic gene clusters; it was thus preferred over a common reporter gene like GFP. (ii) The pig genes do not exhibit any sequence similarity to the genome of P. putida KT2440 that could cause homologous recombination events and would compromise random Tn5 integration into the chromosome. (iii) The gene cluster consists of unidirectionally oriented biosynthetic genes naturally organized in one transcriptional unit23,24, thereby allowing transcription of all genes by a single chromosomal promoter. (vi) All pathway-associated enzymes can be functionally expressed in P. putida and the activation of the prodigiosin biosynthesis in P. putida results in the formation of the red pigment which can be applied as easily quantifiable production readout11,12.
We used the previously constructed plasmid pTREX-pig for conjugational transfer of pig genes to P. putida KT2440. The plasmid carries the complete prodigiosin gene cluster pigA-N and the adjacent gene cueR, which is involved in the intrinsic regulation cascade of S. marcescens but is of minor importance for this study (Fig. 1a). The gene cluster thus also includes the native promoter region of the pigA-N operon; however, when transferred into the heterologous host P. putida and thus in the absence of the complex native regulatory network25,26, it is not functional10. The biosynthetic gene cluster is flanked by the two TREX DNA cassettes which include a gentamicin resistance gene (in R-TREX) as well as the elements of transposon Tn5, enabling random chromosomal integration10,11. To integrate the pig gene cluster at potent expression sites distributed across the host’s chromosome, we followed a workflow previously established for generating P. putida prodigiosin production strains11,12. A library of ca. 50,000 P. putida clones carrying the TREX-pig transposon was generated and screened for clones exhibiting intense red coloration as an indicator of pig gene expression. The total number of screened clones ensured theoretical coverage of the P. putida chromosome comprising 5729 annotated genes with insertions ca. every 248 bp in both strands of the chromosome, assuming that transposition is completely unbiased. We found 50 clones, representing 0.1% of the total number of library clones, showing expression of the prodigiosin pathway indicated by an intense red phenotype, which were designated P. putida pig-r3 to pig-r52 and re-streaked to comparatively evaluate the color phenotype (Fig. 1b). All strains exhibited a very intense red pigmentation except strains pig-r33 and pig-r36, which showed substantially weaker coloration and were therefore excluded from further analysis. In order to corroborate prodigiosin biosynthesis in the new pig-r strains, absorbance spectra of cell extracts derived from representative strains were analyzed after small scale cultivation in liquid TB medium (Fig. 1c). The spectra exhibited an absorption maximum at 535 nm which is typical for prodigiosin11 and indicated that the colored phenotype was indeed caused by accumulation of prodigiosin. In addition, differences in the intensity of the signal gave a first indication that the strains exhibited differential production characteristics. The previously constructed strains P. putida pig-r1 and pig-r211 and the here newly generated strains added up to a set of 50 prodigiosin producing strains that were subjected to detailed analysis of insertion loci and prodigiosin production.
Identification of the rrn operons as insertion loci of pig genes in all pig-r strains
Since we found in our previous study the pig genes to be inserted into the rDNA of P. putida pig-r1 and pig-r2, we first investigated if this was likewise the case for any of the 48 newly generated pig-r strains. To this end, we performed a PCR screen of all strains using a primer pair that would generate a PCR product in case the TREX-pig transposon was inserted in one of the seven rRNA-encoding rrn operons of P. putida KT2440. The seven operons, which are designated rrnA to rrnG, are similarly structured (Fig. 2a) and the promoters as well as the 16S rRNA (1.5 kb) and 23S rRNA (2.9 kb) genes show very high sequence identities (see Supplementary Table S1 for similarity matrices), which are in all cases followed by likewise conserved 5S rRNA genes (Fig. 2a). The operons D, F and G additionally feature tRNA-coding sequences between the 16S and 23S rRNA genes, and operon B contains a second copy of the 5S rRNA gene. Using genomic DNA (gDNA) as template, the 48 newly constructed strains were tested with a forward primer that was designed to bind in the conserved region upstream of the 16S rDNA and a reverse primer binding within the transposon (Fig. 2b and Supplementary Fig. S1; primers AD53 and 54). The gDNA from P. putida pig-r1, pig-r2 and wildtype strain KT2440 were used as positive and negative controls, respectively. As expected, PCR with the wildtype gDNA gave no product, surprisingly however, PCR bands were obtained for all strains carrying the transposon (Supplementary Fig. S2), indicating that the pig genes were inserted into the rDNA in all 50 pig-r strains. Furthermore, the detection of different PCR fragment sizes was a first indication for varying distances of the pig gene insertion sites relative to the primer AD54 binding site located within the promoter regions of all rrn operons.
To verify this and further specify exact insertion loci that were previously also unknown for P. putida pig-r1 and pig-r2, we performed a detailed PCR analysis of all pig-r strains. To this end, seven primers (AD106-112) that specifically bind to the individual upstream regions of the respective rrn operons were used together with the TREX primer AD53 for generating PCR products in strict dependence on the respective TREX-pig insertion site (Supplementary Fig. S1). The operon rrnB represents a special case, as it is preceded by rrnA. Specific PCR bands were obtained for all strains so that insertion into distinct rrn operons could be assigned (Supplementary Fig. S3). The insertion sites were located in all of the seven rrn operons. However, the number of insertion events was not equally distributed: for example, only two strains carrying the TREX-pig transposon in rrnF could be identified, whereas eleven strains carried the recombinant transposon in rrnC. Estimation of PCR product sizes furthermore enabled mapping of each transposon insertion locus within the specific rrn operons and the exact positions were further verified by sequencing of PCR products (Fig. 2a). Figure 2b exemplarily depicts the strategy for the determination of transposon localization in rrnC, and a detailed summary of the methodology and results is given in Supplementary Fig. S1–S3 and Table S2.
In the majority of the tested strains, the insertion site was found to be within a 16S or a 23S rRNA structural gene, without a recognizable pattern therein. P. putida strain pig-r45 represents the only exception where the transposon inserted right before the start of the 16S rRNA structural gene as annotated in the ‘Pseudomonas Genome Database27’. None of the strains carried the pig genes in the region between the rRNA-coding sequences or in the tRNA genes. Interestingly, the fraction of intensely red clones we found after transposition and that were now confirmed to carry the pig genes in the rDNA (0.1%) is in a similar range as the proportion of 16S and 23S rDNA in the genome of P. putida KT2440 (0.25%; the rrn operons A, C and D, which were overrepresented as insertion loci in our sample set and were associated with strongest production, accounting for 0.1% of the genome) (see Supplementary Table S3 for a summary). The 16S and 23S rRNA-coding sequences therefore appear generally promising for integration and expression of a biosynthetic gene cluster.
Correlation of pig gene insertion loci and prodigiosin production
Individual prodigiosin production titers of the 50 P. putida strains carrying the pig genes in the rDNA were analyzed after cultivation in liquid medium to unravel putative correlations with their specific insertion loci. To this end, cells were grown at small scale in TB medium, which was previously determined to be suitable for high-level prodigiosin production11, and end-point product levels were determined after 24 hours based on prodigiosin absorption in ethanol extracts. Afterwards, product titers of the pig-r strains were assigned to the specific rrn operons where pig genes were inserted, and moreover sorted within the respective rrn operon group with respect to the individual distances of the -10 region of the promoters immediately upstream of the 16S rRNA genes to the translation start of the first gene of the pig gene cluster, i.e. pigA (Fig. 3). Note that the minimal possible distance between the start codon of pigA and the rrn promoter is 1.9 kb due to the position and length of the L-TREX cassette and the gene cueR between these two DNA elements (see Fig. 1a).
Based on the set of pig-r strains, several general trends could be observed: (i) Prodigiosin production reached maximal values of ~50–60 mg/L in strains with insertion loci of the pig genes in the rrn operons A, C, D and G, while strains with insertion loci in the rrn operons B, E and F only reached maximal titers of 16–28 mg/L. Evaluation of mean titers of those strains harboring the pig genes within the same rrn operon showed that strains carrying the pig genes in rrn operon A, C and D exhibited generally high prodigiosin accumulation (average ~40 mg/L). In contrast, pig gene insertion in rrn operon B and G resulted in intermediate production levels (average ~25 mg/L) whereas final product titers were even lower in strains with operon E and F as insertion sites (average ~20 mg/L and lower). (ii) Furthermore, in those strains carrying the pig genes within the same rrn operon, a correlation between promotor distance and prodigiosin production becomes apparent: here, a larger distance between the pig genes and the rrn promoter (max. ca. 6.6 kb) mostly correlated with lower production levels whereas shorter distances (min. ca. 2 kb) typically resulted in higher production levels, most clearly for rrn operons A, C and D which are best represented in the data set. This trend seemed especially pronounced in P. putida strains where pig genes were located within in the 16S rRNA gene (see also Supplementary Fig. S4). Interestingly, the strains pig-r33 and pig-r36, which were excluded from our main study due to substantially weaker coloration than the other pig-r strains, accordingly showed a much lower production (below 0.1 mg/L prodigiosin), corroborating our visual assessment, and were tested negative for insertion in the rDNA by the PCR screen.
Since strains with pig gene insertion in some rrn operons were underrepresented in the initially generated set of intense red strains, we additionally created another TREX-pig library comprising ca. 30,000 clones that were specifically tested for gene insertion within the rrn operons B, E, F and G. To this end, we now pre-selected clones with a wider range of colony color phenotypes from light pink to intense red because our above described results (Fig. 3) pointed to lower prodigiosin production by strains with transposon insertion in the underrepresented operons. With these loosened screening criteria, we found a higher fraction of clones within the library to exhibit the target phenotype (1%) than in the initial screening where only very red clones were accepted (0.1%). However, among those exhibiting the target phenotype, the proportion of clones carrying the transposon in the rDNA was significantly lower than in the initial set: out of more than 300 clones with the target phenotype, a random sample of 132 clones was subjected to PCR analysis using the respective primer pairs to indicate the integration into rDNA generally, and into rrn operons B, E, F and G specifically. We found 59 clones to carry the TREX-pig transposon in the rDNA and identified another set of 19 strains with insertion loci in the targeted operons (Supplementary Table S3). Investigation of insertion sites, that were assigned to individual rrn operons on the basis of PCR analysis as described above, and prodigiosin titers corroborated hitherto described trends. Due to the different screening procedure to the main data set (Fig. 3), the results are shown separately (Supplementary Fig. S5).
Our findings thus point to the rDNA as a uniquely suitable chromosomal insertion site for pig gene expression implementing a heterologous prodigiosin pathway and, here, to an influence on production performance depending (i) on the rrn operon, in which pig genes were inserted, and, in addition, (ii) on the distance to the respective rrn promoters. The latter finding is remarkable considering that the total length of the pig gene cluster including cueR is 21.8 kb and a comparably minor difference in promoter distance of few kb or less had a major impact on production levels.
Transcript levels of pig genes inserted into different rDNA loci
To assess if different prodigiosin production titers of P. putida strains with pig gene insertion at different positions in the rDNA were correlated with differential pig gene transcript levels, we exemplarily investigated pig gene mRNA in selected strains. To this end, the transcript of the last gene of the pig gene cluster, pigN, which is most distal to the promoter, was quantified in P. putida strains during cultivation in TB medium by RT-qPCR as an indicator of complete transcription of the entire pig gene cluster (Fig. 4). We first examined the influence of insertion into different rrn operons on pig gene mRNA levels. Therefore, strains carrying pig genes in similar short distances to the promoters (2.4–2.6 kb) of the rrn operons A, C, D, E, F, and G were tested. In addition, two strains with more distal insertions (5.0 kb) in operons A and B were analyzed. Within this data set, a good correlation of pig gene transcript levels and product formation was found (Supplementary Fig. S6), corroborating the role of the individual rrn operons and their promoters for transcription efficiency and thus on final prodigiosin production, except for strain pig-r17, which had a relatively low prodigiosin titer and strain pig-r21, which had a relatively high product titer. Within rrnA, the longer distance to the rrn promoter yielded lower transcript levels, possibly due to increased RNA polymerase drop-off or decreased stability of the mRNA 3′ terminus.
Our results indicate that prodigiosin production appears to be generally correlated to pig gene transcript levels and both, the specific properties of the individual rrn operon as well as the distance between the promoter and the pig gene cluster seem to be key factors determining the level of pathway gene expression in P. putida KT2440.
The expression of bacterial rrn operons is generally thought to be correlated with growth to provide suitable ribosome concentrations matching cellular protein metabolism28 and moreover differentially influenced by environmental factors29,30. Recently, the medium composition has been shown to strongly affect the expression of different rrn operons in E. coli30, with TB rich medium and M9 minimal medium leading to differential expression patterns. For an initial assessment if rrn expression in P. putida might be influenced in a similar way by nutrient limitation, we also tested the minimal medium for comparison of prodigiosin production by selected strains in rich TB vs. minimal M9 medium. Interestingly, product levels were significantly reduced in M9 compared to cultivation in TB medium, but the production pattern was conserved: strains showed the same tendency to group as low-level producers (pig-r17), intermediate producers (pig-r21, -r25, -r35) and high-level producers (pig-r41, -r2) in both media (Supplementary Fig. S7), possibly pointing to intrinsic factors as major determinants of differential rrn operon expression.
The role of the individual rrn operons in determining pig gene transcript levels may be due to (i) differential strength of the seven rrn operon promoters and (ii) distinct effects of their positions in the bacterial chromosome. We therefore further analyzed the upstream sequences of the seven rrn operons of P. putida KT2440 in a comparative alignment to identify specific differences in their promoter sequences (the complete alignment is shown in Supplementary Fig. S8). Although the promoters of the rrn operons have not been characterized specifically for P. putida KT2440 in detail, their positions can be deduced because of their universal nature from sequence similarities to other bacteria and the typical consensus motifs: all upstream regions comprise two potential promoter sequences exhibiting typical -10 and -35 regions of sigma-70 RNA polymerase-dependent promoters as highlighted in yellow and blue, with the one predicted promoter sequence that is located directly upstream of the 16S rRNA gene here denoted as promoter P1 and another one further upstream of the first promoter designated as promoter P2 (Fig. 5a).
Since the exact sequence of the conserved -10 and the -35 regions as well as the spacer region between them are known determinants of promoter activity8,9, the specific differences of these promoter sequences were investigated, using the sequence belonging to rrnA as a reference. In addition, the sequence of the distance regions between the promoter P1 and the 16S rRNA gene, and the sequence between both promoters, here designated as d1 and d2, respectively, were compared (Fig. 5b). The two -10 and -35 regions as well as the spacer region between them are identical for two of the rrn operons (A and D), in which pig gene insertion led to highest production titers (see Fig. 3). The respective sequences of the other rrn operons exhibited different numbers of deviations from the reference, primarily within the sequence of promoter P2. While the promoters of rrnC, which likewise enabled high prodigiosin production titers upon insertion of pig genes, only contain one different nucleotide in a spacer region, those of operons E and F, which were associated with lower product titers, show multiple aberrations not only in the spacer region but also in the -10 and -35 regions. For the same operons, a distance d2 between the two promoter sequences different from all other cases was additionally noted. In contrast to the d1 sequence, where no or only minor aberrations were observed, the d2 sequence moreover harbors moderate (rrnB) and substantial (rrnE and rrnF) aberrations. The overall number of sequence aberrations roughly correlated with production tendencies, i.e. mean and maximal titers, for the six rrn operons A, B, C, D, E and F. However, the promoters and distance sequences d1/d2 of rrnG, which was associated with intermediate production upon pig gene insertion, exhibit only a minor number of total aberrations from the respective sequences of rrnA. In conclusion, the differences in promoter sequences of different rrn operons in the here investigated set of strains carrying the TREX-pig transposon may significantly contribute to the differential transcript and prodigiosin production levels we observed. However, these differences alone cannot account for the observation that some rrn operons appear to be more favorable insertion sites for production than others.
The different genomic contexts of the rrn operons of P. putida KT2440 are likely additional determinants for the efficiency of heterologous gene expression, prompting further inspection. First, the rrn operons are located in individual genomic regions containing different types of upstream sequences in front of their promoters and their expression levels can be affected by various factors including upstream activating sequences, terminators and read-through effects. While their interplay has not been studied for the rrn operons and is difficult to predict, it is conspicuous that genes and consequently the respective promoters upstream of the rrn operons A, C and D, where insertion led to highest production titers, are oriented in the same direction as the rRNA-encoding genes (see Fig. 2a). This might account for potential additional transcriptional read-through – even though ARNold-predicted rho-independent transcription terminators31 occur behind the preceding genes of rrn operons C and D32.
Further, the rrn operons are located at different positions across the chromosome of P. putida KT2440. Since the genomic region in proximity to the origin of chromosomal replication oriC is generally associated with a higher gene dosage33 which may be correlated with gene expression34, we inspected the positions of the rrn operons in relation to the oriC (Fig. 5c). Although the oriC and the corresponding termination dif of P. putida KT2440 have not been characterized in detail, their positions were deduced from sequence similarities to other bacteria35,36,37,38. While the rrn operons A, B, C and D are relatively close to the predicted oriC, the rrn operons E, G and especially F are located at a considerable distance from oriC. The rrn operons F and G are, however, in a similar distance to the terminus of replication, since the proposed oriC and dif regions partition the chromosome in two asymmetrical replicores. With the exception of rrnB, this distribution largely corresponds to the here described production capabilities of strains carrying biosynthetic genes in the rrn operons and might corroborate gene dosage effects. Notably, rrn operons A, B, C, D, E and F are all located in the same replicore, while G is the only one in the other replicore, however, their positions on the (+) and (−) strands, respectively, account for an orientation in the direction of replication in all cases, so that adverse collision effects can be excluded.
Long-term stability of prodigiosin production in P. putida TREX-pig strains
The maintenance of a stable chromosomal integration and the expression performance of biosynthetic genes represents a major challenge in natural products biotechnology7. In general, rDNA appears to be a stably conserved locus39,40. In order to assess the general applicability of P. putida rDNA sites as integration loci in terms of long-term genetic stability and natural product formation, the following strains were subjected to a stability test: (i) P. putida pig-r1 which showed lower production titers and carried the pig genes in the 23S rRNA gene of rrnB, (ii) pig-r2 (intermediate prodigiosin production, insertion in the 16S rRNA gene of rrnC) and (iii) pig-r52 (high prodigiosin production, insertion in the 16S rRNA gene of rrnA) (see Fig. 2a and Fig. 3). To evaluate the long-term stability of these stains, the cell growth and prodigiosin production titers were analyzed after 24 plate-to-plate passages of single colonies over 2 years in direct comparison with strains, which were preserved in cryo-conservation at −80 °C (Fig. 6).
Remarkably, growth and prodigiosin production of the tested strains were basically the same after repeated passaging as compared to cryo-conserved cells. Only minor differences in growth were observed during the exponential phase, but all cell cultures reached the same cell density of ca. 10 (OD650) after 12 h. This corroborates the remarkable resistance of the host to the product prodigiosin, which acts as an antibiotic against other bacteria, and, more importantly, points to the genetic stability and robust expression of clustered genes that are localized within the P. putida rDNA.
In this study, we have described the rRNA-encoding rrn operons of P. putida KT2440 as exceptionally suitable sites to be “hijacked” for recombinant gene cluster insertion and expression. This was demonstrated by (i) selection of prodigiosin producing strains after random chromosomal integration of the pig gene cluster, (ii) substantial but rrn operon-dependent differential expression and prodigiosin production, as well as (iii) a remarkable long-term stability of the TREX-pig containing strains. Our observations indicate that the chromosomal rDNA sites appear to exhibit unique characteristics, which are favorable for effective gene cluster insertion and expression.
A substantial and concerted transcription of biosynthetic genes is necessary to implement a foreign biosynthetic pathway within a heterologous production host. In our study, formation of the desired end product clearly demonstrates that pig gene insertion into the rDNA led to the full transcription of the 21 kb gene cluster, which was confirmed by RT-qPCR analysis of the last gene in the pig cluster. The rrn operons are generally considered to be among the most highly expressed genes in bacteria16. This suggests that biosynthetic genes inserted here can be transcribed at a substantial level as well. Linking heterologous gene cluster transcription to rDNA activation may also grant most efficient use of cellular resources as the transcription of the recombinant biosynthetic genes will occur when the cell is also providing the machinery needed for the protein production. Notably, full transcription in this fashion can only be achieved if the employed gene cluster consists of unidirectionally organized genes with no transcription termination signals in between. In microorganisms, genes coding for large modular biosynthetic pathways are often, like the pig cluster, unidirectionally organized. However, with techniques like recombinational cloning12, gene clusters can otherwise be rearranged to a unidirectional structure. This might, however, compromise a required balance in transcript levels of individual genes and needs to be tested experimentally. Alternative approaches include systematic gene cluster and promoter refactoring which can serve to install beneficial transcription strengths41,42.
We further noted substantial differences of transcription and hence prodigiosin production in dependence of the specific rrn operon carrying the biosynthetic genes, in that the rrn operons A, C and D accounted for highest, B and G for intermediate and E and F for lowest levels, which was largely in concordance with differential promoter sequences. The individual expression levels of the different rrn operons cannot be easily quantified in transcriptome studies due to their high sequence identity so that respective information on the P. putida rrn genes was previously unavailable. Our present study thus provides an initial characterization of cellular processes that hitherto remained a blind spot. For diverse other bacteria including Escherichia coli43 or Lactobacillus plantarum44, varying strength of the different rrn promoters has been reported. Also for Pseudomonads, a differential promoter strength has been indicated29. In addition, a gene dosage effect at locations near the origin of chromosomal replication can be assumed. For E. coli, it was shown that expression levels of genes which are under control of a constitutive promoter correlate with the distance of the genes to the oriC, as more copies of the target genes are available for transcription when they are close to the origin of chromosome replication16,34. This effect can be substantial under the conditions tested, since the majority of cells in a fast-growing P. putida culture have more than two chromosomal copies45. Finally, a co-localization effect of the target biosynthetic genes with the transcription machinery is thinkable: it is known that the transcription and translation machinery represent limited resources in bacterial cells which are subject to competitive interaction by different modules of the cellular circuitry46. Moreover, in P. putida, transcriptional and translational machinery are located in spatially distinct positions in the cell47 and it has been discussed, at least for E. coli, that rrn operons substantially recruit the transcription machinery thus forming transcription foci with high RNA polymerase availability48. Therefore, the transcription level of genes integrated in the rrn operons A–D, which occur in relative proximity to one another, may be especially positively influenced by a local focus of the transcription machinery that is generated here. The thus observed differential expression of the reporter gene cluster inserted into the rrn operons A–G, which led to production differing by a factor of six, may be exploited to implement the optimal expression level for a given biosynthetic pathway.
Overall, a close proximity to the rrn promoter seems to be favorable for higher expression and production levels according to our findings. Assuming that the transcriptional activity for each rrn promoter is not affected by the insertion of the pig construct, the variability in prodigiosin production observed for strains with different insertion loci within one rrn operon could additionally be the result of structural effects on mRNA level. The transcription of the heterologous gene cluster in an rDNA background generally results in an rRNA-mRNA hybrid, where the pig mRNA is flanked by upstream and downstream regions of rRNA fragments. Usually, rRNA remains untranslated and forms secondary structures which are part of the ribosome49,50. Due to these structures, rRNA, unlike mRNA, is exceptionally stable and only degraded under specific conditions51. In an rRNA-mRNA hybrid, extensive base pairing of the flanking rRNA regions thus may co-stabilize the transcript by protecting the mRNA from nuclease activity52. Loop structures formed by the flanking rRNA segments can further improve the accessibility of motifs necessary for efficient translation, e.g. the RBS for proper ribosome recruitment, and enable higher translation rates53. Clones carrying an insertion in the spacer region between the 16S and 23S rRNA genes were not identified. This region is subject to cleavage by several RNases during the process of rRNA maturation49, possibly leading to instable and untranslatable RNA-hybrids. However, interactions between rRNA and mRNA might also have a negative impact on translation rates by blocking sites essential for effective translation. These assumptions are underlined by several outliers, such as strains pig-r32 (Fig. 3) and -r17 (Fig. 4), for which the distance to the promoter clearly is not the only determinant for their production profiles. While promoter proximity is thus certainly a major determinant, local effects can potentially also heavily influence transcript stability and translation efficiency. In future studies, the targeted insertion of gene constructs at the same integration site in the different rrn operons could normalize for these effects, enabling a direct comparison of the transcriptional output of each operon. For the development of a production process, it would be highly interesting to closely study the dynamics of promoter activity, mRNA stability, functional enzyme formation and biosynthetic conversions, and to determine most beneficial constellations. In addition, a systematic assessment with different gene clusters may reveal length- or sequence-specific effects and limitations.
Stable maintenance of biosynthetic DNA is a prerequisite for effective long-term production and a central issue in production strain development. We have shown remarkable stability of prodigiosin producing strains which carry the pig genes in the rDNA. Potentially, the rDNA poses an especially favorable chromosomal site in this regard. Microorganisms seem to have evolved strategies to specifically ascertain correct replication of this essential feature. In bacteria, certain proteins were shown to preferentially associate with the rrn operons in a transcription-dependent manner to cooperatively reduce replication-transcription conflicts at these highly transcribed genes39,54. One might speculate that protective mechanisms specifically directed toward the rDNA might also protect the integrated recombinant genes from accumulating errors during replication. Such phenomena might explain the here observed remarkable stability of prodigiosin producing strains after many generations. However, this idea was not specifically addressed in our study and no control strains with the pig genes inserted in another chromosomal site were subjected to the long-term investigation for comparison. Further studies are necessary to provide evidence on the matter.
Although the discussed unique features recommend the rDNA as highly attractive chromosomal site for gene cluster insertion and expression, disturbing such a vital element of the genome might be expected to exert adverse effects on cellular fitness and production capacities. Indeed, the presence of multiple copies indicates a fundamental importance of rrn genes for bacterial fitness, as shown via artificial reduction of the number of rrn operons in Bacillus15,55. However, we did not observe any apparent fitness defects in our set of strains in the present study and showed in a previous study that growth of P. putida strain pig-r2 in shaking flasks was comparable to that of the wildtype P. putida KT244011. In addition, other P. putida strains such as S12 or S16 only have six rrn operons56,57 with little noticeable effect on the maximum growth rate under laboratory conditions58, indicating a certain plasticity in this trait for the P. putida clade. Likewise, it has been reported elsewhere that the deletion of a single rrn operon of Bacillus subtilis and E. coli does not lead to apparent fitness defects15,59. An explanation for these findings might be that the requirement of a certain number of rrn operons seems to be context-dependent. Specifically, it was suggested that the redundancy of the rrn operon plays a role in the adaptation to different environmental conditions60,61,62 and bacteria with more rrn operon copies are considered more adaptable to changing nutrient availability63,64,65. Under constant laboratory conditions, bacteria appear to compensate the loss of one or two rrn operons by upregulation of others to maintain the required amount of rRNA, as was shown for E. coli66,67.
In summary, our study demonstrates the usability of a natural key feature of the bacterial genome for production strain construction. In the future, expression of biosynthetic pathways in an rDNA context of amenable hosts like P. putida may be used to generate production strains for various natural products. This shall contribute to establishing high-level stable production strains of known compounds, and to the exploitation of yet unknown pathways or silent gene clusters.
Bacterial strains and culture conditions
Escherichia coli strain S17-168, which was applied for conjugation, was cultivated at 37 °C under constant agitation (120 rpm) in shake flasks in liquid LB medium (by Carl Roth®, Karlsruhe, Germany; composed of 10 g/L tryptone, 5 g/L yeast extract, 10 g/L sodium chloride) or on LB agar plates (LB medium completed with 15 g/L Agar-Agar, Kobe I by Carl Roth®). Pseudomonas putida strain KT244013 was cultivated, unless stated otherwise, at 30 °C under constant agitation (120 rpm) in shake flasks in LB liquid medium or on LB agar plates. Antibiotics were supplemented, where appropriate, to the following final concentrations: 10 µg/mL tetracycline (E. coli); 25 µg/mL gentamicin, 25 µg/mL irgasan (P. putida).
Generation of P. putida prodigiosin production strains
Following previously established protocols10,11,12, vector pTREX-pig10, which carries the pig gene cluster from Serratia marcescens W838, was transferred to P. putida KT2440 via conjugation using E. coli S17-1 as donor. Since the origin of replication in pTREX-pig is pMB1, replication is not supported in P. putida. Therefore, positive selection of P. putida clones from the conjugation mix, in which Tn5 transposition of the recombinant TREX-pig transposon comprising the entire prodigiosin biosynthetic pig gene cluster occurred, could be conducted as previously described10,11 by using LB agar plates supplemented with gentamicin because the transposon includes a respective resistance gene. In addition, irgasan was added to selectively allow P. putida growth but prevent E. coli S17-1 growth. Identification of prodigiosin production strains among exconjugants was facilitated by their red colored colony phenotypes on agar plates. Thusly selected clones were streaked on agar plates in distinct patterns to enable a visual comparison of coloration.
Production and quantification of prodigiosin
Prodigiosin production was conducted essentially as previously described11. Prodigiosin producing P. putida strains (P. putida pig-r1 to pig-r52) were grown as precultures in liquid TB medium (by Carl-Roth Karlsruhe, Germany ‘Terrific broth, modified’; composed of 12 g/L Casein, enzymatically digested, 24 g/L yeast extract, 9.4 g/L dipotassium phosphate, 2.2 g/L monopotassium phosphate, 4 mL/L glycerol) or in M9 minimal medium (composed of ‘M9 Minimal Salts’ by Sigma-Aldrich, supplemented with 0.2% glucose, 1 mM MgSO4, 0.1 mM CaCl2, as described by Kurylo et al.30). Production cultures were inoculated from precultures in FlowerPlates® (by m2p-labs GmbH, Baesweiler, Germany) to a starting cell density of OD650 = 0.05 in 800 µL of TB or M9 medium per well. A ThermoMixer® C (by Eppendorf AG, Hamburg, Germany) or a TiMix MTP-shaker with a TH Incubationhood (by EB GmbH, Hechingen, Germany) was used for incubation of production cultures at 20 °C under constant agitation (1400 rpm). Samples with cell masses equivalent to 1 mL cell suspension with a density of OD650 = 0.3–1 (GENESYS™ Spectrophotometer, ThermoFisher Scientific GmbH, Waltham, USA), equivalent to ca. 0.2-0.6 mg dry cell weight, were harvested after 24 h of cultivation by centrifugation. Cells were extracted with 1 mL ethanol (4% of 1 M HCl), cell debris was removed by centrifugation and absorbance spectra from 450 to 600 nm were recorded to verify prodigiosin-specific spectra with the typical maximum at 535 nm. Prodigiosin content in the extracts was determined via the molar extinction coefficient (ε535 [M−1 cm−1] = 139,800) in the solvent as described before11,12 and calculated as prodigiosin titer in mg per liter culture.
Determination of chromosomal integration loci of the TREX-pig transposon within the rDNA
For the determination of the chromosomal integration loci of the TREX-pig transposon in all 50 prodigiosin production strains, a PCR-based method was employed, using Phusion® High-Fidelity DNA-Polymerase (ThermoFisher Scientific GmbH, Waltham, USA) for DNA amplification in a Tprofessional Basis Gradient Thermocycler (Biometra GmbH, Göttingen, Germany). Genomic template DNA was isolated with the DNeasy Blood & Tissue Kit (Quiagen® GmbH, Hilden, Germany). In a first step, integration into any rDNA region was detected by PCR amplification using oligonucleotide AD53, which binds within the L-TREX cassette of the TREX-pig transposon, in combination with oligonucleotide AD54, which binds within the highly conserved upstream regions of every rrn operon and subsequent analysis of PCR products by gel electrophoresis. Genomic DNA was subjected to another PCR to determine the specific rrn operon as well as the accurate integration loci within the genome of P. putida KT2440. Therefore, oligonucleotide AD53 in combination with a specific oligonucleotide for each rrn operon (rrn operon A: AD106, B: AD107, C: AD108, D: AD109, E: AD110, F: AD111, G: AD112) were employed. PCR products were analyzed with agarose gel electrophoresis, isolated using innuPREP DOUBLEpure Kit (Analytik Jena AG, Jena, Germany) and sequenced using oligonucleotide AD134 and AD63. Sequencing results were analyzed based on the Pseudomonas Genome DB27 to verify the assigned rrn operon and to determine the exact integration loci of the TREX-pig transposon. Commercial services were engaged for DNA synthesis of primer oligonucleotides and for DNA sequencing (Eurofins Genomics GmbH, Ebersberg, Germany). Described PCR primer and sequencing primer binding sites are shown in Supplementary Fig. S1 and Fig. 2, respectively. All used oligonucleotides are listed in Supplementary Table S3.
RT-qPCR analysis of transcript levels
Cells were harvested from production cultures during the exponential growth phase (8 h after inoculation, at cell densities of OD650 = 1.5. RNA was extracted from cell material corresponding to OD650 = 1.5 using the NucleoSpin® RNA Kit (Macherey-Nagel). During the procedure, 80 μL DNaseI-Mix (10 μL DNaseI Stock + 70 μL RDD buffer) of the RNase-Free DNase Set (Quiagen) was applied onto the NucleoSpin® RNA column for a 15 min incubation. Total RNA was eluted with 47 μL nuclease-free water and additionally treated with the DNA-free™ DNA Removal Kit (Life Technologies). Reverse transcription was conducted in 20 µL samples using the Maxima First Strand cDNA Synthesis Kit for RT-qPCR (ThermoFisher) with random hexamer primers and 1000 ng RNA as template. After dilution of the samples with water to generate a total volume of 92 µL, 9.2 µL were subjected to qPCR in a reaction mix with 10 µL Maxima SYBR Green/ROX qPCR Master Mix (2×) and 0.8 μL primer mix for the detection of pigN or rpoD transcripts (10 pmol per oligonucleotide), respectively, in the 7900HT Fast Real-Time PCR System running 30 PCR cycles. The primers were designed using the Primer3Web suite69. For calibration, the plasmid pPIG10 was used as template (in concentrations ranging from 1 × 10−3 to 1000 ng), allowing calculation of transcript copy numbers via the molecular weight of detected DNA fragments. Signals of rpoD transcripts were additionally detected as internal reference to monitor RNA extraction and cDNA generation efficiency, and employed for correction of pigN signals by using the deviation of the internal reference signal from the average internal reference signal as a correction factor.
DNA sequence analyses
All P. putida KT2440 genome annotations, sequences and locus tags used for sequence alignments or general analysis were obtained from Pseudomonas Genome DB (http://www.pseudomonas.com)27 using the most recent update (AE015451.2)14 of the P. putida KT2440 genome sequence (AE015451) first published by Nelson et al.13. For multiple sequence alignments, Clustal omega (http://www.ebi.ac.uk/Tools/msa/clustalo/)70 was utilized, for pairwise and global alignments, BLAST (http://blast.ncbi.nlm.nih.gov/)71 was employed. Consensus promotor sequences of the seven rrn operons were predicted with the help of the BPROM analysis tool (http://www.softberry.com/berry.phtml)72; rho-independent terminator sequences were predicted using ARNold (http://rna.igmors.u-psud.fr/toolbox/arnold/)31.
This article does not contain any studies with human participants or animals performed by any of the authors.
All data generated or analyzed during this study are included in this published article (and its Supplementary Information files).
Huo, L. et al. Heterologous expression of bacterial natural product biosynthetic pathways. Nat. Prod. Rep, https://doi.org/10.1039/C8NP00091C (2019).
Nikel, P. I., Chavarría, M., Danchin, A. & de Lorenzo, V. From dirt to industrial applications: Pseudomonas putida as a Synthetic Biology chassis for hosting harsh biochemical reactions. Curr. Opin. Chem. Biol. 34, 20–29 (2016).
Loeschcke, A. & Thies, S. Pseudomonas putida - a versatile host for the production of natural products. Appl. Microbiol. Biotechnol. 99, 6197–6214 (2015).
Martínez-García, E., Aparicio, T., Goñi-Moreno, A., Fraile, S. & De Lorenzo, V. SEVA 2.0: An update of the Standard European Vector Architecture for de-/re-construction of bacterial functionalities. Nucleic Acids Res. 43, D1183–D1189 (2015).
Nikel, P. I., Martínez-García, E. & de Lorenzo, V. Biotechnological domestication of pseudomonads using synthetic biology. Nat. Rev. Microbiol. 12, 368–379 (2014).
Nikel, P. I. & de Lorenzo, V. Pseudomonas putida as a functional chassis for industrial biocatalysis: From native biochemistry to trans-metabolism. Metab. Eng, https://doi.org/10.1016/j.ymben.2018.05.005 (2018).
Zhang, M. M., Wang, Y., Ang, E. L. & Zhao, H. Engineering microbial hosts for production of bacterial natural products. Nat. Prod. Rep. 33, 963–987 (2016).
Zobel, S. et al. Tn7-based device for calibrated heterologous gene expression in Pseudomonas putida. ACS Synth. Biol. 4, 1341–1351 (2015).
Elmore, J. R., Furches, A., Wolff, G. N., Gorday, K. & Guss, A. M. Development of a high efficiency integration system and promoter library for rapid modification of Pseudomonas putida KT2440. Metab. Eng. Commun. 5, 1–8 (2017).
Loeschcke, A. et al. TREX: A universal tool for the transfer and expression of biosynthetic pathways in bacteria. ACS Synth. Biol. 2, 22–33 (2013).
Domröse, A. et al. Efficient recombinant production of prodigiosin in Pseudomonas putida. Front. Microbiol. 6, 972 (2015).
Domröse, A. et al. Rapid generation of recombinant Pseudomonas putida secondary metabolite producers using yTREX. Synth. Syst. Biotechnol. 2, 310–319 (2017).
Nelson, K. E. et al. Complete genome sequence and comparative analysis of the metabolically versatile Pseudomonas putida KT2440. Environ. Microbiol. 4, 799–808 (2002).
Belda, E. et al. The revisited genome of Pseudomonas putida KT2440 enlightens its value as a robust metabolic chassis. Environ. Microbiol. 18, 3403–3424 (2016).
Yano, K. et al. Multiple rRNA operons are essential for efficient cell growth and sporulation as well as outgrowth in Bacillus subtilis. Microbiology 159, 2225–2236 (2013).
Rocha, E. P. C. The replication-related organization of bacterial genomes. Microbiology 150, 1609–1627 (2004).
Mitra, P., Ghosh, G., Hafeezunnisa, M. & Sen, R. Rho Protein: Roles and Mechanisms. Annu. Rev. Microbiol. 71, 687–709 (2017).
Belasco, J. G. All things must pass: contrasts and commonalities in eukaryotic and bacterial mRNA decay. Nat. Rev. Mol. Cell Biol. 11, 467–748 (2010).
Deutscher, M. P. How bacterial cells keep ribonucleases under control. FEMS Microbiol. Rev. 39, 350–361 (2015).
Lewenza, S. et al. Construction of a mini-Tn5-luxCDABE mutant library in Pseudomonas aeruginosa PAO1: A tool for identifying differentially regulated genes. Genome Res. 15, 583–589 (2005).
Choi, K.-H. & Kim, K.-J. Applications of transposon-based gene delivery system in bacteria. J. Microbiol. Biotechnol. 19, 217–228 (2009).
Reznikoff, W. S. Transposon Tn 5. Annu. Rev. Genet. 42, 269–286 (2008).
Harris, A. K. P. et al. The Serratia gene cluster encoding biosynthesis of the red antibiotic, prodigiosin, shows species- and strain-dependent genome context variation. Microbiology 150, 3547–60 (2004).
Williamson, N. R., Fineran, P. C., Leeper, F. J. & Salmond, G. P. C. The biosynthesis and regulation of bacterial prodiginines. Nat. Rev. Microbiol. 4, 887–99 (2006).
Stella, N. A. et al. Serratia marcescens cyclic AMP receptor protein controls transcription of eepR, a novel regulator of antimicrobial secondary metabolites. J. Bacteriol. 197, 2468–2478 (2015).
Wilf, N. M. et al. RNA-seq reveals the RNA binding proteins, Hfq and RsmA, play various roles in virulence, antibiotic production and genomic flux in Serratia sp. ATCC 39006. BMC Genomics 14, 822 (2013).
Winsor, G. L. et al. Enhanced annotations and features for comparing thousands of Pseudomonas genomes in the Pseudomonas genome database. Nucleic Acids Res. 44, D646–D653 (2016).
Bosdriesz, E., Molenaar, D., Teusink, B. & Bruggeman, F. J. How fast-growing bacteria robustly tune their ribosome concentration to approximate growth-rate maximization. FEBS J. 282, 2029–2044 (2015).
Duan, J., Reimer, L., Heikkila, J. J. & Glick, B. R. Differential expression of the seven rRNA operon promoters from the plant growth-promoting bacterium Pseudomonas sp. UW4. FEMS Microbiol. Lett. 361, 181–189 (2014).
Kurylo, C. M. et al. Endogenous rRNA sequence variation can regulate stress response gene expression and phenotype. Cell Rep. 25, 236–248.e6 (2018).
Lesnik, E. A. et al. Prediction of rho-independent transcriptional terminators in Escherichia coli. Nucleic Acids Res. 29, 3583–5894 (2001).
Cambray, G. et al. Measurement and modeling of intrinsic transcription terminators. Nucleic Acids Res. 41, 5139–5148 (2013).
Slager, J. & Veening, J.-W. Hard-wired control of bacterial processes by chromosomal gene location. Trends Microbiol. 24, 788–800 (2016).
Block, D. H. S., Hussein, R., Liang, L. W. & Lim, H. N. Regulatory consequences of gene translocation in bacteria. Nucleic Acids Res. 40, 8979–8992 (2012).
Yee, T. W. & Smith, D. W. Pseudomonas chromosomal replication origins: a bacterial class distinct from Escherichia coli-type origins. Proc. Natl. Acad. Sci. USA 87, 1278–1282 (1990).
Wolanski, M., Donczew, R., Zawilak-Pawlik, A. & Zakrzewska-Czerwinska, J. oriC-encoded instructions for the initiation of bacterial chromosome replication. Front. Microbiol. 5, 735 (2015).
Carnoy, C. & Roten, C.-A. The dif/Xer recombination systems in proteobacteria. PLoS One 4, e6531 (2009).
Aparicio, T., Jensen, S. I., Nielsen, A. T., de Lorenzo, V. & Martínez-García, E. The Ssr protein (T1E_1405) from Pseudomonas putida DOT-T1E enables oligonucleotide-based recombineering in platform strain P. putida EM42. Biotechnol. J. 11, 1309–1319 (2016).
Merrikh, H., Zhang, Y., Grossman, A. D. & Wang, J. D. Replication-transcription conflicts in bacteria. Nat. Rev. Microbiol. 10, 449–458 (2012).
Kobayashi, T. Ribosomal RNA gene repeats, their stability and cellular senescence. Proc. Japan Acad. Ser. B 90, 119–129 (2014).
Horbal, L., Marques, F., Nadmid, S., Mendes, M. V. & Luzhetskyy, A. Secondary metabolites overproduction through transcriptional gene cluster refactoring. Metab. Eng. 49, 299–315 (2018).
Kim, S. et al. Atolypenes, tricyclic bacterial sesterterpenes discovered using a multiplexed in vitro Cas9-TAR gene cluster refactoring approach. ACS Synth. Biol. 8, 109–118 (2019).
Maeda, M., Shimada, T. & Ishihama, A. Strength and regulation of seven rRNA promoters in Escherichia coli. PLoS One 10, e0144697 (2015).
Rud, I., Jensen, P. R., Naterstad, K. & Axelsson, L. A synthetic promoter library for constitutive gene expression in Lactobacillus plantarum. Microbiology 152, 1011–1019 (2006).
Lieder, S. et al. Subpopulation-proteomics reveal growth rate, but not cell cycling, as a major impact on protein composition in Pseudomonas putida KT2440. AMB Express 4, 71 (2014).
Qian, Y., Huang, H. H., Jiménez, J. I. & Del Vecchio, D. Resource competition shapes the response of genetic circuits. ACS Synth. Biol. 6, 1263–1272 (2017).
Kim, J., Goñi-Moreno, A., Calles, B. & de Lorenzo, V. Spatial organization of the gene expression hardware in Pseudomonas putida. Environ. Microbiol, https://doi.org/10.1111/1462-2920.14544 (2019).
Cabrera, J. E. & Jin, D. J. Active transcription of rRNA operons is a driving force for the distribution of RNA polymerase in bacteria: Effect of extrachromosomal copies of rrnB on the in vivo localization of RNA polymerase. J. Bacteriol. 188, 4007–4014 (2006).
Deutscher, M. P. Maturation and Degradation of Ribosomal RNA in Bacteria. In Progress in Molecular Biology and Translational Science (ed. Condon, C.) 369–391, https://doi.org/10.1016/S0079-6603(08)00809-X (Elsevier Inc., 2009).
Petrov, A. S. et al. Secondary structures of rRNAs from all three domains of life. PLoS One 9, e88222 (2014).
Deutscher, M. P. Degradation of RNA in bacteria: Comparison of mRNA and stable RNA. Nucleic Acids Res. 34, 659–666 (2006).
Rauhut, R. & Klug, G. mRNA degradation in bacteria. FEMS Microbiol. Rev. 23, 353–370 (1999).
Carrier, T. A. & Keasling, J. D. Engineering mRNA stability in E. coli by the addition of synthetic hairpins using a 5′ cassette system. Biotechnol. Bioeng. 55, 577–580 (1997).
Lang, K. S. & Merrikh, H. The clash of macromolecular titans: Replication-transcription conflicts in bacteria. Annu. Rev. Microbiol. 72, 71–88 (2018).
Nanamiya, H. et al. Bacillus subtilis mutants harbouring a single copy of the rRNA operon exhibit severe defects in growth and sporulation. Microbiology 156, 2944–2952 (2010).
Kuepper, J., Ruijssenaars, H. J., Blank, L. M., de Winde, J. H. & Wierckx, N. Complete genome sequence of solvent-tolerant Pseudomonas putida S12 including megaplasmid pTTS12. J. Biotechnol. 200, 17–18 (2015).
Yu, H. et al. Complete genome sequence of the nicotine-degrading Pseudomonas putida strain S16. J. Bacteriol. 193, 5541–5542 (2011).
Blank, L. M., Ionidis, G., Ebert, B. E., Bühler, B. & Schmid, A. Metabolic response of Pseudomonas putida during redox biocatalysis in the presence of a second octanol phase. FEBS J. 275, 5173–5190 (2008).
Ellwood, M. & Nomura, M. Deletion of a ribosomal ribonucleic acid operon in. Escherichia coli. J. Bacteriol. 143, 1077–1080 (1980).
Gyorfy, Z. et al. Engineered ribosomal RNA operon copy-number variants of E. coli reveal the evolutionary trade-offs shaping rRNA operon number. Nucleic Acids Res. 43, 1783–1794 (2015).
Elser, J. J. et al. Biological stoichiometry from genes to ecosystems: ideas, plans, and realities. Ecol. Lett. 3, 540–550 (2000).
Green, J. L., Bohannan, B. J. M. & Whitaker, R. J. Microbial Biogeography: From Taxonomy to Traits. Science. 320, 1039–1044 (2008).
Valdivia-Anistro, J. A. et al. Variability of rRNA operon copy number and growth rate dynamics of Bacillus isolated from an extremely oligotrophic aquatic ecosystem. Front. Microbiol. 6, 1486 (2016).
Klappenbach, J. A., Saxman, P. R., Cole, J. R. & Schnidt, T. M. Rrndb: the ribosomal RNA operon copy number database. Nucleic Acids Res. 29, 181–184 (2001).
Elser, J. J. Biological stoichiometry: A theoretical framework connecting ecosystem ecology, evolution, and biochemistry for application in astrobiology. Int. J. Astrobiol. 2, 185–193 (2003).
Jinks-Robertson, S., Gourse, R. L. & Nomura, M. Expression of rRNA and tRNA genes in Escherichia coli: Evidence for feedback regulation by products of rRNA operons. Cell 33, 865–876 (1983).
Condon, C., French, S., Squires, C. & Squires, C. L. Depletion of functional ribosomal RNA operons in Escherichia coli causes increased expression of the remaining intact copies. EMBO J. 12, 4305–4315 (1993).
Simon, R., Priefer, U. & Pühler, A. A broad host range mobilization system for in vivo genetic engineering: transposon mutagenesis in Gram negative bacteria. Nat. Biotechnol. 1, 784–791 (1983).
Untergasser, A. et al. Primer3-new capabilities and interfaces. Nucleic Acids Res. 40, e115 (2012).
Sievers, F. et al. Fast, scalable generation of high-quality protein multiple sequence alignments using Clustal Omega. Mol. Syst. Biol. 7, 539 (2011).
Altschul, S. F., Gish, W., Miller, W., Myers, E. W. & Lipman, D. J. Basic local alignment search tool. J. Mol. Biol. 215, 403–410 (1990).
Solovyev, V. & Salamov, A. Automatic Annotation of Microbial Genomes and Metagenomic Sequences. In Metagenomics and its Applications in Agriculture, Biomedicine and Environmental Studies (ed. Li, R. W.) 61–78 (Nova Science Publishers, 2011).
We gratefully acknowledge the Ministry of Culture and Science of the German Federal State of North Rhine-Westphalia and the Heinrich Heine University Düsseldorf for a scholarship to A.D. within the CLIB Graduate Cluster Industrial Biotechnology. S.T., R.W. and A.L. were funded by the Ministry of Culture and Science of the German State of North Rhine-Westphalia through NRW Strategieprojekt BioSC (No. 313/323-400-00213). J.H.H. was funded by the German Research Foundation DFG within CEPLAS – the Cluster of Excellence on Plant Sciences (EXC1028). N.W. and M.O. were funded by the German Research Foundation DFG through the Emmy Noether program (WI 4255/1-1).
The authors declare no competing interests.
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Domröse, A., Hage-Hülsmann, J., Thies, S. et al. Pseudomonas putida rDNA is a favored site for the expression of biosynthetic genes. Sci Rep 9, 7028 (2019). https://doi.org/10.1038/s41598-019-43405-1
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