- Open Access
Low-mutation-rate, reduced-genome Escherichia coli: an improved host for faithful maintenance of engineered genetic constructs
© Csörgő et al; licensee BioMed Central Ltd. 2012
- Received: 19 October 2011
- Accepted: 20 January 2012
- Published: 20 January 2012
Molecular mechanisms generating genetic variation provide the basis for evolution and long-term survival of a population in a changing environment. In stable, laboratory conditions, the variation-generating mechanisms are dispensable, as there is limited need for the cell to adapt to adverse conditions. In fact, newly emerging, evolved features might be undesirable when working on highly refined, precise molecular and synthetic biological tasks.
By constructing low-mutation-rate variants, we reduced the evolutionary capacity of MDS42, a reduced-genome E. coli strain engineered to lack most genes irrelevant for laboratory/industrial applications. Elimination of diversity-generating, error-prone DNA polymerase enzymes involved in induced mutagenesis achieved a significant stabilization of the genome. The resulting strain, while retaining normal growth, showed a significant decrease in overall mutation rates, most notably under various stress conditions. Moreover, the error-prone polymerase-free host allowed relatively stable maintenance of a toxic methyltransferase-expressing clone. In contrast, the parental strain produced mutant clones, unable to produce functional methyltransferase, which quickly overgrew the culture to a high ratio (50% of clones in a 24-h induction period lacked functional methyltransferase activity). The surprisingly large stability-difference observed between the strains was due to the combined effects of high stress-induced mutagenesis in the parental strain, growth inhibition by expression of the toxic protein, and selection/outgrowth of mutants no longer producing an active, toxic enzyme.
By eliminating stress-inducible error-prone DNA-polymerases, the genome of the mobile genetic element-free E. coli strain MDS42 was further stabilized. The resulting strain represents an improved host in various synthetic and molecular biological applications, allowing more stable production of growth-inhibiting biomolecules.
- Escherichia coli
- mutation rate
- reduced genome
- synthetic biology
Intrinsic mechanisms for generating diversity are important for survival of bacterial populations in dynamically changing environmental conditions. The ability of a population to adapt to various situations is largely dependent upon a constant fine-tuning of mutation rate . However, what is beneficial in a natural environment is not necessary when conditions are relatively stable and controlled, as in laboratory and industrial settings. In fact, novel, evolved features arising in a carefully designed and fabricated system of biological parts can lead to unwanted genotypic and phenotypic alterations, and the spontaneous genetic modification of an established production strain or a clone library is usually highly undesirable . Consequently, whether used as a production strain, a cloning host, or as a synthetic biological chassis, a bacterial cell with increased genetic stability is of great importance [3–5].
In addition to being a universal cloning host, Escherichia coli is the most common organism used in the production of proteins, metabolites, and secondary metabolites, for both research and industrial purposes [6–12]. In an effort to improve the performance of these 'workhorse' strains, several large-scale modifications have been made to various E. coli strains using genome engineering methods [13–17]. These efforts all follow the basic principle of streamlining metabolic pathways for the increased production of a given biomaterial coupled with reduction of unwanted byproducts. Along these lines, a reduced-genome E. coli strain (MDS42) was constructed in our laboratories. Most genes irrelevant for laboratory applications, as well as all known mobile DNA sequences and cryptic virulence genes were precisely deleted, resulting in a genetically stabilized strain that displays several advantageous properties . The advantages of using an MDS42 background for industrial purposes was demonstrated by increased L-threonine production in a modified version of the multi-deletion strain . In a recent work, we have also shown that the IS element-free MDS42 host improves maintenance of unstable genetic constructs, allowing for stable cloning of certain toxic genes .
Evidence exists that some genes, in their functional forms, are unusually difficult to clone in bacterial plasmids, and aberrant clones frequently arise [21–24]. Normally, the general mutation rate of the host cell is so low (~10-7 mutation/gene/generation) , that spontaneous changes in a cloned DNA fragment are extremely rare and therefore cannot solely account for the cloning artifacts. However, when the cloned DNA fragment interferes with normal cell physiology and reduces growth, the rare mutants of the clone can be positively selected for and can rapidly become dominant in the culture. This phenomenon became apparent to us in an earlier attempt to clone the VP60 gene of rabbit hemorrhagic virus . VP60 fused to a cholera toxin component proved to be toxic to the cell. Inactivation of the recombinant gene due to IS element-transposition and insertion into the toxic gene, followed by rapid selection of the mutants, resulted in only aberrant clones in normal E. coli cloning hosts. Using the MDS42 host cell free of all IS elements, the recombinant gene could be cloned in its intact form.
Here we wish to expand this work by making further improvements on the genetic stability of MDS42. Beyond the previous elimination of all IS insertion events, we disabled other mutation-generating pathways of the host in order to improve tolerance and fidelity. Removal of IS elements from the host genome eliminated a major, sometimes dominant  form of mutation generation. However, in many cases, toxic clones are inactivated by point mutations or deletions. A detailed analysis of clones of hepatitis C virus genes showed that the cloning procedure in E. coli resulted exclusively in defective, non-expressing clones due to the selection of point mutants (either frameshifts or stop codons) . Selection of defective forms of toxic genes can be so effective, that it can actually be used deliberately to obtain point mutants, as demonstrated by isolation of mutants of human immunodeficiency virus protease  or of the PvuII DNA methyltransferase . Unlike insertion mutagenesis by IS elements, point mutations as a whole cannot be totally eliminated. Nevertheless, any reduction in mutation rate expands the cloning potential of the host cell and improves its function as a synthetic biological chassis.
Our strategy for reducing point mutation rate in E. coli involved disabling the effective mutation generating enzymes of the SOS response. Under stressful conditions (e.g. toxic clones harbored in the cell), DNA damage may occur, activating the SOS response, inducing approximately 40 members of the SOS regulon [29–32]. Three of the genes induced during the SOS response of E. coli encode DNA polymerases (Pol II, Pol IV, Pol V) that are able to bypass replication barriers at damaged sites and stalled replication forks [33–36]. All three of the SOS-inducible polymerases have been implicated in induced mutagenesis , with Pol IV and Pol V having error-rates approximately 2 to 3 orders of magnitude higher than the high-fidelity replicative polymerase (Pol III) . Pol II, while showing high fidelity on undamaged templates, was shown to take part in certain types of stress-induced mutagenesis [37, 39, 40]. The SOS-regulated polymerases are dispensable; their primary role seems to be the generation of genetic diversity under stressful conditions . DNA repair has alternative pathways, most notably recombination-mediated repair, which can rescue stalled replication in a less error-prone manner .
We show here that the disabling of stress-induced mutagenesis mechanisms further increases the genetic stability of MDS42, a reduced-genome E. coli strain lacking all mobile genetic elements. We offer proof of the beneficial effects of the resulting strain as a cloning host in the stable maintenance of a toxic gene. The improved strain shows promising potential as a cellular chassis for molecular and synthetic biological applications.
The absence of error-prone polymerases reduces the spontaneous mutation rate
The genes coding for the three error-prone DNA polymerases (polB, dinB, umuDC) were deleted from the genome of MDS42 in a scarless manner using a suicide plasmid-based method . Gene deletions were made individually and also joined in all possible combinations. The spontaneous mutation rate of each strain was then determined using a D-cycloserine resistance assay, detecting all types of mutations in the cycA gene .
As an additional measure of fitness, we analyzed the survival rate of MDS42pdu and MDS42 in long-term stationary phase (Additional file 1). No significant difference was observed between the two strains over a period of 7 days. Furthermore, when the two strains were additionally stressed by expressing a moderately toxic protein from the pSin32 plasmid (discussed later), the survival rates in stationary phase were not significantly different either.
Inactivation of the regulators of the SOS response does not lower the spontaneous mutation rate
MDS42pdu is genetically stable under stress conditions
Due to the stress-induced nature of the error-prone DNA polymerases, it was expected that the difference in mutation rates of the polymerase-free and the parent strain would be even more pronounced under stressful conditions. Mutation rates were therefore measured under stressful conditions, including the application of an antibiotic agent (mitomycin-C), overproduction of benign Green Fluorescent Protein (GFP) [49, 50], and overproduction of a toxic protein (ORF238) .
Mitomycin-C, a DNA cross-linking agent that causes lesions in double-stranded DNA , directly activates the SOS response, leading to the up-regulation of error-prone DNA polymerase enzymes. A sub-inhibitory concentration (0.1 μg/ml) of mitomycin-C was used to stress the cells and analyze the effect on mutation rates. Protein overproduction imposes stress on the host cell [52, 53]. To test the effect of overproduction on mutation rates, genes for either non-toxic GFP, or the toxic small, leucine-rich hydrophobic protein ORF238  were cloned on plasmids as inducible constructs controlled by a T7 promoter. To express them, T7 RNA polymerase encoding variants of the studied strains were constructed. Fitness measurements of these modified strains revealed no significant decrease compared to MDS42 (Additional file 2). In addition to MDS42pdu and its parent MDS42, the widely used protein production strain BL21(DE3), the wild-type K-12 MG1655, and also the two different SOS-inactivated variants of MDS42 (MDS42recA and MDS42lexA(S119A)) were tested (Figure 4).
Results showed that, with the exception of MDS42recA and MDS42pdu, the various stresses generally increased the mutation rate. Overproduction of the toxic ORF238 protein had the largest effect: a > 5-fold increase in mutation rate was measured. Sub-inhibitory concentration of mitomycin-C caused a > 2-3-fold increase in the mutation rate (BL21(DE3) and MDS42recA were unable to grow under these conditions). The overproduction of GFP had a minor effect, a 1.5 to 2-fold increase in mutation rate.
In contrast, no significant increase in mutation rate in the presence of any of the stressors could be seen in either MDS42recA or MDS42pdu. (Interestingly, MDS42lexA(S119A) did not follow this behavior, the strain showed an increase in mutation rate in response to all of the stresses.) MDS42pdu can be characterized as the genetically most stable strain, displaying the lowest spontaneous mutation rate and showing negligible response to stressful conditions.
To confirm the data obtained using the cycA fluctuation assay, mutation rates of MDS42 and MDS42pdu under each of the different stress conditions were also measured using a second assay. The data obtained using the rifampicin resistance assay (detecting point mutations in the essential rpoB gene ) were consistent with the cycA fluctuation assay data (Additional file 3). MDS42pdu had a 2-fold lower spontaneous mutation frequency compared to MDS42. In response to the overproduction of the toxic ORF238 protein, as well as in the presence of mitomycin-C, the mutation rate of MDS42 became significantly elevated, while the response of MDS42pdu was much less substantial.
The error-prone polymerase-free strain provides improved stability to a toxic protein-expressing plasmid clone
In order to demonstrate the practical advantage of working with a strain of higher genome stability, a plasmid-based mutation screen was designed. Plasmid pSin32 carries an inducible copy of sinI, coding for the SinI methyltransferase of Salmonella enterica serovar Infantis. SinI methylates the inner cytosines in DNA at GG(A/T)CC sites, producing 5-methylcytosine, thereby creating targets for the McrBC endonuclease, which cleaves DNA containing methylcytosine. A plasmid that carries methylated SinI sites (e.g., pSin32, self-methylated at its 8 SinI sites), therefore cannot establish itself in a mcrBC+ host. To check what ratio of an induced pSin32 sample carries mutated sinI (not expressing a functional SinI), the plasmid sample is transformed in both MDS42 (McrBC-) and MG1655 (McrBC+), and colony numbers are compared (see methods).
Surprisingly, 96.7% of the starting (0-hour) plasmid sample, originating from MDS42, could not be established in MG1655. This indicated that, even in a host lacking T7 polymerase, spurious transcription of sinI had resulted in SinI expression, and consequently, methylation of SinI sites. The methylated status of the SinI sites in the original plasmid sample was confirmed by their uncleavability by SinI (data not shown).
Differences regarding clone stability in the different strains became evident after IPTG-induction of SinI expression. Thirty-six hours after transformation (28 hours after IPTG-induction), 51.7% of pSin32 harbored in BL21(DE3)mcrBC cells carried mutations preventing the production of active SinI. This value was significantly lower in MDS42-T7 (25.8%, p < 0.005 with a two-tailed, unpaired t-test). In MDS42pdu-T7, the fraction of mutated pSin32 plasmids was even lower (8.2%, p < 0.005). The non-methylated status of the SinI sites on the plasmids carrying a mutated sinI gene was confirmed by their cleavability by SinI (data not shown).
It seemed evident, that accumulation of mutant plasmids in BL21(DE3)mcrBC and MDS42-T7 was due to a combined effect of stress-induced mutagenesis and growth inhibition by the SinI-expressing plasmid. Production of the enzyme elevated mutation rates and reduced growth. In these slow-growing cultures, over time, SinI-inactivating mutations arose, which then, having resumed their normal growth rate, quickly overgrew the rest of the culture. In the low-mutation-rate MDS42pdu- T7, SinI-inactivating mutations developed, on average, over a longer time period. Growth curve measurements of 50 independent colonies of MDS42-T7 and MDS42pdu-T7, all carrying the pSin32 plasmid, support this notion. An O.D.540 value of 0.7 was used as a cutoff to indicate that a culture had overcome the growth-hindering effect of the induced plasmid. The average time taken for MDS42pdu- T7 to reach this level of density was significantly longer than for MDS42-T7 (727.8 and 571.8 minutes, respectively; P < 0.005, two-tailed, unpaired t test).
To verify that mutations had indeed taken place in the plasmids that allowed for growth in McrBC+ cells, the sinI region of 8 different plasmid samples (taken from viable, pSin32-transformed MG1655 colonies) were sequenced (Additional file 4). In seven out of the eight cases, a frameshift mutation had occurred in sinI, resulting in a new stop codon within the gene. The eighth case displayed an A to C transversion, resulting in the N255T mutation of the protein. Six out of the seven new stop codons caused by the frameshifts were located within the first 125 bp of the gene.
One of the major challenges that synthetic biology must face is the intrinsic variability and genetic instability of living organisms . As the complexity of synthetic systems increase, the emergence and selection of new features will become a significant impediment in achieving robust and stable performance. Improving the genetic stability of the host organism, or synthetic biological chassis is therefore a validated goal.
Previously, we have demonstrated that genome stabilization by elimination of mobile genetic elements has advantages in certain cloning applications [18, 20]. To achieve additional genetic stabilization of the host, we targeted and eliminated error-prone DNA polymerases (Pol II, Pol IV, Pol V), major sources of frameshift and point mutations. Possible alternative approaches to lower the mutation rate include the introduction of a so-called antimutator dnaE allele or upstream inactivation of the SOS response by introducing a recA or lexA mutation. Previous studies on the effect of antimutators found a 5 to 30 fold reduction in mutation rate . It was later shown that the mode of action of these DnaE antimutators was a more effective ability to exclude error-prone DNA polymerases at sites of DNA synthesis during DSB-repair associated stress-induced mutagenesis , suggesting that the elimination of these enzymes would reproduce the antimutator effect. Testing the other alternative approaches, MDS42recA, compared to MDS42pdu, showed a much less pronounced reduction in spontaneous mutation rate. Furthermore, owing to the central role of the RecA enzyme in cell physiology , unwanted pleiotropic effects might arise within the cell, manifested, among others, in sensitivity to mitomycin-C, presumably due to insufficient repair activity. MDS42lexA(S119A), carrying a non-cleavable form of the LexA repressor, did not significantly lower the mutation rate under the conditions applied. The small effect of the recA and lexA mutations can be explained by the relative SOS-independence of the error-prone polymerases: the enzymes are present even in unstressed cells, and can be up-regulated by a number of (not just SOS) stress responses (Figure 1) .
Several studies have been made on the effects of error-prone polymerases on mutation rates using various strains of E. coli and various methods of measurement. Supporting our findings is the observation that deletion of dinB significantly decreases the mutation rates for both frameshift and base substitution mutations in a Lac+ reversion system, as well as in a rifampicin resistance assay . In another study, the lack of Pol V caused a decrease in the number of Arg+ growth dependent revertants . Later studies also showed that post-exposure mutation rates in the presence of ciprofloxacin were markedly reduced when all three inducible polymerases were separately eliminated .
Here, using a D-cycloserine resistance-based fluctuation analysis , confirmed in some cases by a rifampicin resistance assay as well, we carefully quantified the effect of individual and combined error-prone polymerase deletions on the mutation rate, under either unstressed or stressed conditions. We determined that, under unstressed conditions, elimination of each error-prone polymerase by itself significantly decreased the spontaneous mutation rate. The effect of combining deletions ΔpolB and ΔdinB was additive, indicating an independent mode of action for these polymerases. However, ΔumuDC generated no additional decrease of the mutation rate when any of the other two error prone polymerases was missing, possibly marking an interaction among the genes or their products. This phenomenon has been described previously regarding ΔdinB and ΔumuDC, the nature of their putative interaction, however is not yet known .
As expected, the most dramatic differences in mutation rate between MDS42 and MDS42pdu were observed under various stress conditions. A sub-inhibitory concentration of the SOS response-activating mitomycin-C, overproduction of either the non-toxic GFP protein or of the highly toxic ORF238 hydrophobic protein all significantly increased the mutation rate of MDS42. The values for MDS42pdu remained stable under the same conditions. It is also noteworthy, that among the strains tested, the commonly used production strain BL21(DE3) showed not just the highest spontaneous mutation rate, but also the highest increase in mutation rates in response to the various stresses. A difference of almost two orders of magnitude was observed between the mutation rate of BL21(DE3) and MDS42pdu when overproducing the toxic ORF238 protein. This elevated rate of mutation in BL21(DE3) can be mostly attributed to an increased rate of IS insertions.
A clear practical advantage of working with MDS42pdu was demonstrated in a protein production experiment, where the SinI methyltransferase was expressed from an inducible plasmid construct. SinI, producing 5-methylcytosines is toxic to cells that carry the McrBC endonuclease. Even in cells lacking McrBC, we observed a negative effect on cell fitness. When SinI was produced, we found that the sinI gene, carried on a plasmid, acquired loss-of-function mutations approximately three times less frequently in MDS42pdu than in MDS42, and over five times less frequently than in BL21(DE3)mcrBC. Remarkably, after only 16 hours of production in BL21(DE3)mcrBC, almost half of all sinI genes encoded on the plasmids had suffered a disabling mutation.
Clearly, the unexpectedly high ratio of mutated clones in the SinI-expressing culture cannot be explained solely by the stress-induced mutagenesis, the overall mutation rate of which being too low in absolute values (in the order of 10-6 mutations/gene/generation) to cause such a dramatic effect. Rather, the phenomenon is in large part due to the growth inhibitory effect of the plasmid carrying the toxic gene. The chain of events is the following: Upon induction of expression of the toxic gene, growth rate of the cell is reduced. At the same time, mutation rate is increased by the stress. Once a mutant, not producing the toxic protein, arises in the plasmid population, the cell harboring it can resume normal growth and become dominant in the culture. In low-mutation-rate MDS42pdu, appearance of such mutants is delayed, and the cells can produce the functional toxic protein for an extended period of time.
Calculating the precise advantage of MDS42pdu over the parental MDS42 or the commonly used production strain BL21(DE3) can be challenging, due to the stochastic nature of mutagenesis, as well as the lack of exact data on the fitness cost of overproduction. Nevertheless, it is clear that the more severe the stress of overproducing a product is (resulting in an elevated mutation rate and growth inhibition), the greater the advantage of the stabilized host.
The mutation and inactivation of engineered genetic constructs within a host cell is an overlooked problem that may have serious detrimental effects on the success of any synthetic biological, molecular biological or biotechnological process. A gene product imposing a metabolic burden or being toxic to the host drives an evolutionary force that selects for any mutants that alleviate the growth-inhibiting effect. A host cell or chassis with enhanced genetic stability is advantageous in the stable maintenance of these constructs. By eliminating the error-prone DNA polymerase enzymes from the reduced-genome MDS42 strain lacking all genomic IS elements, we have further stabilized a strain that already showed clear advantages in cloning applications. The resulting MDS42pdu strain had a significant stabilizing effect on a toxic protein expression clone. This high-fidelity strain, producing decreased genetic variation in the culture, might also prove useful in applications ranging from the production of DNA therapeutics to long-term continuous fermentation processes.
Strains, plasmids, media, and oligonucleotide primers
Genomic coordinates of each scarless deletion.
Coordinates of deletion
Growth properties were evaluated in liquid medium in 100-well Honeycomb 2 plates (Oy Growth Curves Ab, Helsinki, Finland). Growth curves were measured by following the optical densities (O.D.) at 540 nm in each well using the Bioscreen C Automated Microbiology Growth Analysis System (Oy Growth Curves Ab, Helsinki, Finland). Fourteen individual colonies from each strain type were resuspended and grown in parallel to saturation at 37°C in MOPS medium. From the saturated cultures, 2 μl was transferred to 198 μl fresh MOPS medium and grown to saturation in individual wells at 37°C using continuous shaking. The median O.D. value of the fourteen parallel cultures corresponding to each strain was calculated and plotted for each time point. Doubling times were calculated from these growth curves using previously described methods . For analysis of growth in the presence of the SinI methyltransferase, 50 resuspended individual colonies of MDS42-T7 and MDS42pdu-T7, each harboring the pSin32 plasmid, were grown to saturation in LB medium supplemented with 50 μg/ml ampicillin. From the saturated cultures, 2 μl was transferred to 198 μl of fresh LB and ampicillin and grown to O.D. = 0.2, then IPTG inducer was added at a final concentration of 1 mM. An O.D.540 value of 0.7 was arbitrarily chosen as a point where the culture had overcome the toxic effect of SinI. The duration of the growth inhibition for each sample was averaged for both strains.
To measure long-term survival of individual strains, 5 ml LB cultures were inoculated 1:1000 (vol:vol) from fresh overnight cultures. Viable counts were determined directly from the cultures incubated at 37°C for up to one week.
Mutation rate measurements
D-cycloserine resistance assays were performed as previously described . Briefly, in a fluctuation assay, 20 tubes of 1 ml MS medium  supplemented with 0.2% glucose were inoculated with approximately 104 cells each, and cultures were grown to early stationary phase. Aliquots of 50 μl from each tube were then spread on MS plates containing D-cycloserine (0.04 mM). The number of mutations per tube (m) was estimated from the number of colonies by fluctuation analysis using the Ma-Sandri-Sarkar maximum-likelihood method . Equation 41 from the report of Stewart et al.  was used to extrapolate the obtained m value, valid for 50 μl, to 1 ml. Statistical comparisons of m values were made only when the difference in total cell number was negligible (< 3%, P ≤ 0.6, with a two-tailed, unpaired t test). The total number of cells in a tube was calculated by spreading dilutions from three random tubes onto nonselective plates. Dividing the number of mutations per tube by the average total number of cells in a tube gave the mutational rate (mutation/gene/generation). To assess the effect of the antibiotic mitomycin-C on mutation rate, 0.1 μg/ml of mitomycin-C was added to each tube. When measuring mutation rates of cells harboring a protein-overproducing plasmid, cultures were induced with 1 mM IPTG at an O.D.540 value of 0.2. In these cases the selective antibiotic for the specific plasmid was also present in the MS medium.
In a second protocol, to confirm data obtained using the cycA assay, cells resistant to rifampicin (carrying mutations in rpoB ) were selected and counted. Twenty tubes of 1 ml LB were inoculated with 104 cells each, and cultures were grown to early stationary phase. Appropriate dilutions were spread onto non-selective LB agar plates and LB agar plates containing rifampicin (100 μg/ml). Colony counts were performed after 24 or 48 h, respectively. Mutation frequencies were reported as a proportion of the number of rifampicin-resistant colonies relative to the total viable count. The results correspond to the mean value obtained in three independent experiments for each strain and condition. When required, different stress conditions were provided in the same manner as in the cycA assay.
Analysis of mutational spectra
Analysis of the mutational spectrum of the cycA gene has been described previously . In brief, a 1877-bp genomic segment encompassing the entire gene was amplified from mutant cells using the primer pair cycA-D/cycA-E. A representative sample was obtained by analyzing 5 colonies from each parallel plate, yielding a total of 96 samples per experiment. The amplified fragments were resolved on an agarose gel and compared to a fragment generated from the wild-type template. Identical sizes indicated a mutation affecting only one or a few nucleotides, a decrease in size or failure of amplification indicated a deletion, and a detectable increase in size indicated an IS insertion.
Assay to detect mutations in sinI
Plasmid pSin32 carries the gene sinI coding for SinI methyltransferase of Salmonella enterica serovar Infantis cloned into the XhoI site of the pET3-His plasmid . The plasmid was electroporated into MDS42-T7, MDS42pdu-T7 and BL21(DE3)mcrBC. After 1 hour of recovery incubation at 37°C in 1 ml LB, 100 μl of the transformed cultures were placed in 100 ml LB supplemented with Ap and incubated at 37°C. From the remaining 900 μl, plasmid DNA was isolated according to standard protocols . After 7 hours of incubation, the cultures reached O.D.540 = ~0.2, at which point the samples were induced with IPTG (1 mM final concentration). Samples for plasmid preparation were also taken at this time (8-hour samples), followed by additional samples being taken every 2 hours, up to 18 hours, then at 24 and 36 hours of post-transformation growth. Purified pSin32 plasmid samples (9 from each strain) were then transformed into MDS42 (McrBC-) and MG1655 (McrBC+). By counting transformed MG1655 and MDS42 colonies for each plasmid sample, the relative number of mutated plasmids could be calculated. To obtain an absolute value for mutated plasmid numbers, each batch of electrocompetent MDS42 and MG1655 indicator strains was transformed with a control (pST76-A) plasmid  carrying an Ap resistance cassette. The ratio of MG1655 and MDS42 transformants was then used as a correcting factor to calculate absolute values for the number of mutated pSin32 plasmids for each sample.
We thank John W. Campbell for the critical reading of the manuscript, Antal Kiss for the pSin32 plasmid construct, and Gabriella Balikó, Ildikó Karcagi, and Ágnes Szalkanovics for technical assistance. This project was supported by the Hungarian Research Fund (OTKA K43260 and OTKA PD72719) and the European Community's Seventh Framework Program (FP7/2007-2013) under grant agreement no. 212894. TF is supported by the Bolyai Foundation.
- Denamur E, Matic I: Evolution of mutation rates in bacteria. Mol Microbiol 2006,60(4):820-827. 10.1111/j.1365-2958.2006.05150.xView ArticleGoogle Scholar
- Endy D: Foundations for engineering biology. Nature 2005,438(7067):449-453. 10.1038/nature04342View ArticleGoogle Scholar
- Chou CP: Engineering cell physiology to enhance recombinant protein production in Escherichia coli. Appl Microbiol Biotechnol 2007,76(3):521-532. 10.1007/s00253-007-1039-0View ArticleGoogle Scholar
- Gao H, Zhuo Y, Ashforth E, Zhang L: Engineering of a genome-reduced host: practical application of synthetic biology in the overproduction of desired secondary metabolites. Protein Cell 2010,1(7):621-626. 10.1007/s13238-010-0073-3View ArticleGoogle Scholar
- Andrianantoandro E, Basu S, Karig DK, Weiss R: Synthetic biology: new engineering rules for an emerging discipline. Mol Syst Biol 2006, 2: 2006 0028.View ArticleGoogle Scholar
- Arbabi-Ghahroudi M, Tanha J, MacKenzie R: Prokaryotic expression of antibodies. Cancer Metastasis Rev 2005,24(4):501-519. 10.1007/s10555-005-6193-1View ArticleGoogle Scholar
- Baneyx F: Recombinant protein expression in Escherichia coli. Curr Opin Biotechnol 1999,10(5):411-421. 10.1016/S0958-1669(99)00003-8View ArticleGoogle Scholar
- Jana S, Deb JK: Strategies for efficient production of heterologous proteins in Escherichia coli. Appl Microbiol Biotechnol 2005,67(3):289-298. 10.1007/s00253-004-1814-0View ArticleGoogle Scholar
- Jarboe LR, Zhang X, Wang X, Moore JC, Shanmugam KT, Ingram LO: Metabolic engineering for production of biorenewable fuels and chemicals: contributions of synthetic biology. J Biomed Biotechnol 2010, 2010: 761042.View ArticleGoogle Scholar
- Meagher RB, Tait RC, Betlach M, Boyer HW: Protein expression in E. coli minicells by recombinant plasmids. Cell 1977,10(3):521-536. 10.1016/0092-8674(77)90039-3View ArticleGoogle Scholar
- Sorensen HP, Mortensen KK: Advanced genetic strategies for recombinant protein expression in Escherichia coli. J Biotechnol 2005,115(2):113-128. 10.1016/j.jbiotec.2004.08.004View ArticleGoogle Scholar
- Terpe K: Overview of bacterial expression systems for heterologous protein production: from molecular and biochemical fundamentals to commercial systems. Appl Microbiol Biotechnol 2006,72(2):211-222. 10.1007/s00253-006-0465-8View ArticleGoogle Scholar
- Cebolla A, Royo JL, De Lorenzo V, Santero E: Improvement of recombinant protein yield by a combination of transcriptional amplification and stabilization of gene expression. Appl Environ Microbiol 2002,68(10):5034-5041. 10.1128/AEM.68.10.5034-5041.2002View ArticleGoogle Scholar
- Chevalet L, Robert A, Gueneau F, Bonnefoy JY, Nguyen T: Recombinant protein production driven by the tryptophan promoter is tightly controlled in ICONE 200, a new genetically engineered E. coli mutant. Biotechnol Bioeng 2000,69(4):351-358. 10.1002/1097-0290(20000820)69:4<351::AID-BIT1>3.0.CO;2-GView ArticleGoogle Scholar
- Ferrer-Miralles N, Domingo-Espin J, Corchero JL, Vazquez E, Villaverde A: Microbial factories for recombinant pharmaceuticals. Microb Cell Fact 2009, 8: 17. 10.1186/1475-2859-8-17View ArticleGoogle Scholar
- Chou CH, Bennett GN, San KY: Genetic manipulation of stationary-phase genes to enhance recombinant protein production in Escherichia coli. Biotechnol Bioeng 1996,50(6):636-642. 10.1002/(SICI)1097-0290(19960620)50:6<636::AID-BIT4>3.0.CO;2-LView ArticleGoogle Scholar
- Mizoguchi H, Mori H, Fujio T: Escherichia coli minimum genome factory. Biotechnol Appl Biochem 2007,46(Pt 3):157-167.Google Scholar
- Posfai G, Plunkett G, Feher T, Frisch D, Keil GM, Umenhoffer K, Kolisnychenko V, Stahl B, Sharma SS, de Arruda M, et al.: Emergent properties of reduced-genome Escherichia coli. Science 2006,312(5776):1044-1046. 10.1126/science.1126439View ArticleGoogle Scholar
- Lee JH, Sung BH, Kim MS, Blattner FR, Yoon BH, Kim JH, Kim SC: Metabolic engineering of a reduced-genome strain of Escherichia coli for L-threonine production. Microb Cell Fact 2009, 8: 2. 10.1186/1475-2859-8-2View ArticleGoogle Scholar
- Umenhoffer K, Feher T, Baliko G, Ayaydin F, Posfai J, Blattner FR, Posfai G: Reduced evolvability of Escherichia coli MDS42, an IS-less cellular chassis for molecular and synthetic biology applications. Microb Cell Fact 2010, 9: 38. 10.1186/1475-2859-9-38View ArticleGoogle Scholar
- Rood JI, Sneddon MK, Morrison JF: Instability in tyrR strains of plasmids carrying the tyrosine operon: isolation and characterization of plasmid derivatives with insertions or deletions. J Bacteriol 1980,144(2):552-559.Google Scholar
- Kumar PK, Maschke HE, Friehs K, Schugerl K: Strategies for improving plasmid stability in genetically modified bacteria in bioreactors. Trends Biotechnol 1991,9(8):279-284.View ArticleGoogle Scholar
- Amster O, Salomon D, Zamir A: A cloned immunoglobulin cDNA fragment enhances transposition of IS elements into recombinant plasmids. Nucleic Acids Res 1982,10(15):4525-4542. 10.1093/nar/10.15.4525View ArticleGoogle Scholar
- Forns X, Bukh J, Purcell RH, Emerson SU: How Escherichia coli can bias the results of molecular cloning: preferential selection of defective genomes of hepatitis C virus during the cloning procedure. Proc Natl Acad Sci USA 1997,94(25):13909-13914. 10.1073/pnas.94.25.13909View ArticleGoogle Scholar
- Drake JW, Charlesworth B, Charlesworth D, Crow JF: Rates of spontaneous mutation. Genetics 1998,148(4):1667-1686.Google Scholar
- Hall BG: Activation of the bgl operon by adaptive mutation. Mol Biol Evol 1998,15(1):1-5.View ArticleGoogle Scholar
- Baum EZ, Bebernitz GA, Gluzman Y: Isolation of mutants of human immunodeficiency virus protease based on the toxicity of the enzyme in Escherichia coli. Proc Natl Acad Sci USA 1990,87(14):5573-5577. 10.1073/pnas.87.14.5573View ArticleGoogle Scholar
- Blumenthal RM, Cotterman MM: Isolation of mutants in a DNA methyltransferase through mcrB-mediated restriction. Gene 1988,74(1):271-273.Google Scholar
- Radman M: SOS repair hypothesis: phenomenology of an inducible DNA repair which is accompanied by mutagenesis. Basic Life Sci 1975, 5A: 355-367.Google Scholar
- Quillardet P, Rouffaud MA, Bouige P: DNA array analysis of gene expression in response to UV irradiation in Escherichia coli. Res Microbiol 2003,154(8):559-572. 10.1016/S0923-2508(03)00149-9View ArticleGoogle Scholar
- Fernandez De Henestrosa AR, Ogi T, Aoyagi S, Chafin D, Hayes JJ, Ohmori H, Woodgate R: Identification of additional genes belonging to the LexA regulon in Escherichia coli. Mol Microbiol 2000,35(6):1560-1572.View ArticleGoogle Scholar
- Wade JT, Reppas NB, Church GM, Struhl K: Genomic analysis of LexA binding reveals the permissive nature of the Escherichia coli genome and identifies unconventional target sites. Genes Dev 2005,19(21):2619-2630. 10.1101/gad.1355605View ArticleGoogle Scholar
- Reuven NB, Arad G, Maor-Shoshani A, Livneh Z: The mutagenesis protein UmuC is a DNA polymerase activated by UmuD', RecA, and SSB and is specialized for translesion replication. J Biol Chem 1999,274(45):31763-31766. 10.1074/jbc.274.45.31763View ArticleGoogle Scholar
- Bonner CA, Randall SK, Rayssiguier C, Radman M, Eritja R, Kaplan BE, McEntee K, Goodman MF: Purification and characterization of an inducible Escherichia coli DNA polymerase capable of insertion and bypass at abasic lesions in DNA. J Biol Chem 1988,263(35):18946-18952.Google Scholar
- Tang M, Pham P, Shen X, Taylor JS, O'Donnell M, Woodgate R, Goodman MF: Roles of E. coli DNA polymerases IV and V in lesion-targeted and untargeted SOS mutagenesis. Nature 2000,404(6781):1014-1018. 10.1038/35010020View ArticleGoogle Scholar
- Wagner J, Gruz P, Kim SR, Yamada M, Matsui K, Fuchs RP, Nohmi T: The dinB gene encodes a novel E. coli DNA polymerase, DNA pol IV, involved in mutagenesis. Mol Cell 1999,4(2):281-286. 10.1016/S1097-2765(00)80376-7View ArticleGoogle Scholar
- Napolitano R, Janel-Bintz R, Wagner J, Fuchs RP: All three SOS-inducible DNA polymerases (Pol II, Pol IV and Pol V) are involved in induced mutagenesis. EMBO J 2000,19(22):6259-6265. 10.1093/emboj/19.22.6259View ArticleGoogle Scholar
- Tippin B, Pham P, Goodman MF: Error-prone replication for better or worse. Trends Microbiol 2004,12(6):288-295. 10.1016/j.tim.2004.04.004View ArticleGoogle Scholar
- Frisch RL, Su Y, Thornton PC, Gibson JL, Rosenberg SM, Hastings PJ: Separate DNA Pol II- and Pol IV-dependent pathways of stress-induced mutation during double-strand-break repair in Escherichia coli are controlled by RpoS. J Bacteriol 2010,192(18):4694-4700. 10.1128/JB.00570-10View ArticleGoogle Scholar
- Wagner J, Etienne H, Janel-Bintz R, Fuchs RP: Genetics of mutagenesis in E. coli: various combinations of translesion polymerases (Pol II, IV and V) deal with lesion/sequence context diversity. DNA Repair (Amst) 2002,1(2):159-167. 10.1016/S1568-7864(01)00012-XView ArticleGoogle Scholar
- Yeiser B, Pepper ED, Goodman MF, Finkel SE: SOS-induced DNA polymerases enhance long-term survival and evolutionary fitness. Proc Natl Acad Sci USA 2002,99(13):8737-8741.View ArticleGoogle Scholar
- Berdichevsky A, Izhar L, Livneh Z: Error-free recombinational repair predominates over mutagenic translesion replication in E. coli. Mol Cell 2002,10(4):917-924. 10.1016/S1097-2765(02)00679-2View ArticleGoogle Scholar
- Lin LL, Little JW: Isolation and characterization of noncleavable (Ind-) mutants of the LexA repressor of Escherichia coli K-12. J Bacteriol 1988,170(5):2163-2173.Google Scholar
- Cirz RT, Chin JK, Andes DR, de Crecy-Lagard V, Craig WA, Romesberg FE: Inhibition of mutation and combating the evolution of antibiotic resistance. PLoS Biol 2005,3(6):e176. 10.1371/journal.pbio.0030176View ArticleGoogle Scholar
- Foster PL: Stress-induced mutagenesis in bacteria. Crit Rev Biochem Mol Biol 2007,42(5):373-397. 10.1080/10409230701648494View ArticleGoogle Scholar
- Little JW, Edmiston SH, Pacelli LZ, Mount DW: Cleavage of the Escherichia coli lexA protein by the recA protease. Proc Natl Acad Sci USA 1980,77(6):3225-3229. 10.1073/pnas.77.6.3225View ArticleGoogle Scholar
- Feher T, Karcagi I, Gyorfy Z, Umenhoffer K, Csorgo B, Posfai G: Scarless engineering of the Escherichia coli genome. Methods Mol Biol 2008, 416: 251-259. 10.1007/978-1-59745-321-9_16View ArticleGoogle Scholar
- Feher T, Cseh B, Umenhoffer K, Karcagi I, Posfai G: Characterization of cycA mutants of Escherichia coli. An assay for measuring in vivo mutation rates. Mutat Res 2006,595(1-2):184-190. 10.1016/j.mrfmmm.2005.11.004View ArticleGoogle Scholar
- Deschamps JR, Miller CE, Ward KB: Rapid purification of recombinant green fluorescent protein using the hydrophobic properties of an HPLC size-exclusion column. Protein Expr Purif 1995,6(4):555-558. 10.1006/prep.1995.1073View ArticleGoogle Scholar
- Shimomura O, Johnson FH, Saiga Y: Extraction, purification and properties of aequorin, a bioluminescent protein from the luminous hydromedusan, Aequorea. J Cell Comp Physiol 1962, 59: 223-239. 10.1002/jcp.1030590302View ArticleGoogle Scholar
- Tomasz M, Palom Y: The mitomycin bioreductive antitumor agents: cross-linking and alkylation of DNA as the molecular basis of their activity. Pharmacol Ther 1997,76(1-3):73-87. 10.1016/S0163-7258(97)00088-0View ArticleGoogle Scholar
- Hoffmann F, Rinas U: Stress induced by recombinant protein production in Escherichia coli. Adv Biochem Eng Biotechnol 2004, 89: 73-92.Google Scholar
- Gasser B, Saloheimo M, Rinas U, Dragosits M, Rodriguez-Carmona E, Baumann K, Giuliani M, Parrilli E, Branduardi P, Lang C, et al.: Protein folding and conformational stress in microbial cells producing recombinant proteins: a host comparative overview. Microb Cell Fact 2008, 7: 11. 10.1186/1475-2859-7-11View ArticleGoogle Scholar
- Jin DJ, Gross CA: Mapping and sequencing of mutations in the Escherichia coli rpoB gene that lead to rifampicin resistance. J Mol Biol 1988,202(1):45-58. 10.1016/0022-2836(88)90517-7View ArticleGoogle Scholar
- Kwok R: Five hard truths for synthetic biology. Nature 2010,463(7279):288-290. 10.1038/463288aView ArticleGoogle Scholar
- Fijalkowska IJ, Dunn RL, Schaaper RM: Mutants of Escherichia coli with increased fidelity of DNA replication. Genetics 1993,134(4):1023-1030.Google Scholar
- Hastings PJ, Hersh MN, Thornton PC, Fonville NC, Slack A, Frisch RL, Ray MP, Harris RS, Leal SM, Rosenberg SM: Competition of Escherichia coli DNA polymerases I, II and III with DNA Pol IV in stressed cells. PLoS One 2010,5(5):e10862. 10.1371/journal.pone.0010862View ArticleGoogle Scholar
- Lusetti SL, Cox MM: The bacterial RecA protein and the recombinational DNA repair of stalled replication forks. Annu Rev Biochem 2002, 71: 71-100. 10.1146/annurev.biochem.71.083101.133940View ArticleGoogle Scholar
- Strauss BS, Roberts R, Francis L, Pouryazdanparast P: Role of the dinB gene product in spontaneous mutation in Escherichia coli with an impaired replicative polymerase. J Bacteriol 2000,182(23):6742-6750. 10.1128/JB.182.23.6742-6750.2000View ArticleGoogle Scholar
- Nowosielska A, Janion C, Grzesiuk E: Effect of deletion of SOS-induced polymerases, pol II, IV, and V, on spontaneous mutagenesis in Escherichia coli mutD5. Environ Mol Mutagen 2004,43(4):226-234. 10.1002/em.20019View ArticleGoogle Scholar
- Yamada M, Nunoshiba T, Shimizu M, Gruz P, Kamiya H, Harashima H, Nohmi T: Involvement of Y-family DNA polymerases in mutagenesis caused by oxidized nucleotides in Escherichia coli. J Bacteriol 2006,188(13):4992-4995. 10.1128/JB.00281-06View ArticleGoogle Scholar
- Blattner FR, Plunkett G, Bloch CA, Perna NT, Burland V, Riley M, Collado-Vides J, Glasner JD, Rode CK, Mayhew GF, et al.: The complete genome sequence of Escherichia coli K-12. Science 1997,277(5331):1453-1462. 10.1126/science.277.5331.1453View ArticleGoogle Scholar
- Miller JH: Experiments in Molecular Genetics. Cold Spring Harbor, NY: Cold Spring Harbor Laboratory Press; 1972.Google Scholar
- Chen BP, Hai T: Expression vectors for affinity purification and radiolabeling of proteins using Escherichia coli as host. Gene 1994,139(1):73-75. 10.1016/0378-1119(94)90525-8View ArticleGoogle Scholar
- Timar E, Venetianer P, Kiss A: In vivo DNA protection by relaxed-specificity SinI DNA methyltransferase variants. J Bacteriol 2008,190(24):8003-8008. 10.1128/JB.00754-08View ArticleGoogle Scholar
- Sambrook J, Fritch EF, Maniatis T: Molecular Cloning. A laboratory manual. Cold Spring Harbor, NY: Cold Spring Harbor Laboratory Press; 1987.Google Scholar
- Warringer J, Ericson E, Fernandez L, Nerman O, Blomberg A: High-resolution yeast phenomics resolves different physiological features in the saline response. Proc Natl Acad Sci USA 2003,100(26):15724-15729. 10.1073/pnas.2435976100View ArticleGoogle Scholar
- Sarkar S, Ma WT, Sandri GH: On fluctuation analysis: a new, simple and efficient method for computing the expected number of mutants. Genetica 1992,85(2):173-179. 10.1007/BF00120324View ArticleGoogle Scholar
- Stewart FM, Gordon DM, Levin BR: Fluctuation analysis: the probability distribution of the number of mutants under different conditions. Genetics 1990,124(1):175-185.Google Scholar
- Posfai G, Koob MD, Kirkpatrick HA, Blattner FR: Versatile insertion plasmids for targeted genome manipulations in bacteria: isolation, deletion, and rescue of the pathogenicity island LEE of the Escherichia coli O157:H7 genome. J Bacteriol 1997,179(13):4426-4428.Google Scholar
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