Overexpression of the third H-NS paralogue H-NS2 compensates fitness loss in hns mutants of the enteroaggregative Escherichia coli strain 042

Members of the H-NS protein family play a role both in the chromosome architecture and in the regulation of gene expression in bacteria. The genomes of the enterobacteria encode an H-NS paralogue, the StpA protein. StpA displays specific regulatory properties and provides a molecular backup for H-NS. Some enterobacteria also encode third H-NS paralogues. This is the case of the enteroaggregative E. coli (EAEC) strain 042, which encodes the hns, stpA and hns2 genes. We provide in this paper novel information about the role of the H-NS2 protein in strain 042. A C > T transition in the hns2 promoter leading to increased H-NS2 expression is readily selected in hns mutants. Increased H-NS2 expression partially compensates for H-NS loss. H-NS2 levels are critical for the strain 042 fitness. Under some circumstances, high H-NS2 expression levels dictated by the mutant hns2 promoter can be deleterious. The selection of T > C revertants or of clones harboring insertional inactivations of the hns2 gene can then occur. Temperature also plays a relevant role in the H-NS2 regulatory activity. At 37 °C, H-NS2 targets a subset of the H-NS repressed genes contributing to their silencing. When temperature drops to 25 °C, the repressory ability of H-NS2 is significantly reduced. At low temperature, H-NS plays the main repressory role.

www.nature.com/scientificreports/ pSF-R27 provides a stealth function, avoiding the fact that plasmid incorporation results in a fitness cost for the bacterial host 24 . Some pathogenic E. coli strains can also encode additional hns paralogues. The uropathogenic strain 536 encodes a third hns paralogue, the hfp gene 25 . The main regulatory role of the Hfp protein was found to occur at temperatures outside the host (25 °C). The H-NS paralogues StpA, Sfh and Hfp have been proposed to modulate H-NS activity by forming heteromers with H-NS, which display DNA-binding properties different from those from homomeric H-NS [25][26][27] . The enteroaggregative E. coli strain 042 also contains a third H-NS paralogue, termed H-NS2 28 . The H-NS2 protein shows 64.4% identity with the H-NS protein. H-NS2 displays specific expression and regulatory properties. H-NS2 targets at 37 °C only a subset of those genes that are regulated by H-NS, and may help to differentially regulate core and HGT genes by the H-NS cellular pool 28 . We present in this report further information about the biological role of the H-NS2 protein. The H-NS2 expression levels can be modified by a spontaneous reversible C > T transition in the promoter region of the hns2 gene. In strain 042 hns mutants, increased H-NS2 expression partially compensates for H-NS loss when cells grow at low temperature. We also show a differential regulatory role of the H-NS2 protein at 25 °C and 37 °C.

Results
Passaging of strain 042 Δhns derivatives for 10 days at 25 °C generates cultures with increased growth rate. In different enterobacterial strains, loss of H-NS function results in a reduced growth rate. An experimental evolution approach designed to identify secondary mutations compensating for H-NS loss in Salmonella showed that, when subculturing Δhns mutants, some of the Δhns cell lineages that increased the growth rate accumulated mutations in the stpA gene, generating StpA variants with altered DNA binding and oligomerization properties, resembling those of H-NS 29 . We considered that a similar approach could be performed with strain 042 in order to gain insight into H-NS2 function. We hypothesized that, as it was the case with the stpA gene in Salmonella Δhns mutants 29 , subcultures of a Δhns derivative of the E. coli strain 042 would generate clones with increased fitness, which could harbor mutations mapping either in the hns2 or in the stpA genes.
We already checked that Δhns mutants of strain 042 show a reduced growth rate, especially when cells grow at low temperature 28 . For the directed evolution experiment, three independent cultures of strain 042 Δhns were serially passaged alongside one lineage of the WT strain in LB medium and were grown either at 37 °C or at 25 °C for 10 days. Each day aliquots were diluted 1:1.000 for cultures grown at 37 °C, and 1:100 for cultures grown at 25 °C. At days 1, 5 and 10, aliquots were frozen at -80 °C for retrospective analysis of the genetic changes in each lineage over time. At days 1, 5, and 10 growth curves were determined both for the WT and for the different Δhns lineages (Fig. 1A,B). Cultures grown at 37 °C and 25 °C showed different patterns. Although the number of generations of cultures grown at 37 °C was significantly higher than that of cultures grown at 25 °C, Δhns lineages grown at 37 °C did not display significant increases in their growth rates compared to that of the day 1 clone. In contrast, all three Δhns lineages grown at 25 °C displayed significant increases in the growth rate at day 5 and reached values similar to that of the WT clone at day 10 (Table 1A,B).
The three Δhns lineages subcultured at 25 °C contain the same mutation in the hns2 gene. With the aim to correlate the observed increase in the growth rate in the Δhns subcultures with alterations in either the hns2 or the stpA genes, we used first the 10 days old lineages of the WT and Δhns mutant lineage 1 cultured at 25 °C to amplify by PCR and sequence the hns2 and stpA genes. All three Δhns lineages showed no alterations in the stpA gene, but they contained the same mutation in the hns2 gene: a C > T transition in the predicted promoter region, specifically located in the last position of the -10 box (hereon termed phns2* promoter) ( Fig. 2A). We also studied the kinetics of the appearance of the C > T transition at 25 °C in all three Δhns lineages by analyzing the hns2 promoter sequence in all 5-and 10-days old subcultures (Fig. 2B). In the 5 days old subcultures of clone 1, most of the cells already showed the C > T transition. Subcultures of clones 2 and 3 contained mixtures of cells containing both the WT and mutant hns2 promoters. In the 10 days old subcultures, the C nucleotide had been totally replaced by T in all three clones (Fig. 2B). Taking into account that the identified mutation occurs within the hns2 promoter region, we decided to identify the transcriptional start point of the hns2 gene. We used 5′ RACE to map the + 1 transcriptional start site of the hns2 gene in strains 042 WT, 042 Δhns and 042 Δhns phns2*. In all three strains, transcription is initiated at a G residue, 7 nucleotides downstream of the -10 box and 41 nucleotides upstream of the hns2 start codon ( Supplementary Fig. S1).
To rule out that other genetic changes out of the hns2 promoter mutation were underlying the increased growth rate of the Δhns mutant, the genomes of both the WT 042 strain and one of the 10 days old Δhns subculture were sequenced. No other significant genomic alterations (i.e., deletions of specific DNA regions) were detected.
In the E. coli strain MG1655, in vitro evolution experiments performed with a double hns stpA mutant revealed that either point mutations inactivating the sigma factor RpoS or an amplification of ∼40% of the chromosome centered around the origin of replication could partially compensate the physiological alterations caused by the simultaneous loss of H-NS and StpA 30 . We decided to assess whether similar changes could be selected in a 042 double hns stpA mutant. To our surprise, the double hns stpA mutant showed a similar growth rate than that of the WT strain. We sequenced then the hns2 gene in the hns stpA mutant strain. It contains the same identified C > T transition in the promoter region.
The identified mutation in the hns2 promoter increases H-NS2 expression. The likely explanation for the relationship between the C > T transition in the mutant hns2 promoter and the increased growth rate of the 10 days old subcultures of the Δhns mutants at 25 °C is that the H-NS2 expression is higher in the Δhns clone harboring the phns2* promoter than in the Δhns clone harboring the WT phns2 promoter. www.nature.com/scientificreports/ this, we studied both hns2 transcription and H-NS2 expression in clones harboring respectively the WT phns2 and mutant phns2* promoters.
To assess the transcriptional activity of the WT and phns2* promoters, they were cloned in the pFZY1 plasmid and transformed in the strain 042 ΔlacZ. Samples from cultures of strains 042 ΔlacZ (pFZY1phns2) and 042 ΔlacZ (pFZY1phns2*) grown in LB medium both at 25 °C and at 37 °C were collected at the exponential (OD 600 0.4) and the early stationary (OD 600 2.0) growth phases, and the β-galactosidase activity was determined (Fig. 3A). As expected, the β-galactosidase activity of cells harboring the phns2* promoter is higher than that of cells harboring the WT phns2 promoter in all samples analyzed.
To correlate the transcriptional activity dictated by both phns2 and phns2* promoters with protein expression, a Flag-tag was added to the C-terminal end of the hns2 gene of strains 042 WT, 042 Δhns and 042 Δhns phns2*.   (Fig. 3B). As previously reported 28 , H-NS2 is overexpressed in an Δhns mutant. As expected, H-NS2 levels are higher in strain Δhns phns2* than in strain 042 Δhns. We also analyzed the phns2* sequence by using the BPROM software. This analysis showed that a recognition sequence for the CpxR transcription factor is generated in the phns2* promoter ( Supplementary Fig. S2). CpxR is the two-component response regulator that is sensitive to phosphorylation by CpxA. This two-component www.nature.com/scientificreports/ system responds to, among other environmental factors, periplasm and outer membrane stress 31 . We decided to study whether the mutant promoter phns2* was activated by CpxR. To that end, we obtained a ΔcpxR derivative of strain 042 ΔlacZ. The ΔlacZ ΔcpxR derivative was transformed with plasmids pZYF1phns2 and pZYF1phns2*. The presence of the cpxR allele did not modify the induction of the transcription of the lacZ gene under the control of the phns2* promoter ( Supplementary Fig. S3).  www.nature.com/scientificreports/ to that of the WT strain ( Fig. 4). This suggests that pLGhns2-dependent H-NS2 expression levels compensate either for H-NS or H-NS/H-NS2 loss. In contrast, the growth rate of strain 042 Δhns (pLGhns2*) was lower than that of the Δhns mutant and the growth rate of strain Δhns Δhns2 (pLGhns2*) was higher than that of strain Δhns Δhns2, but significantly lower than that of the WT strain. This shows that expression of H-NS2 dictated by plasmid pLGhns2* is not compensating for H-NS loss. To clarify this, we amplified by PCR and sequenced the hns2 gene from strains 042 Δhns (pLGhns2) and 042 Δhns (pLGhns2*). PCR amplification of the hns2 gene in the former strain generated a single band, and the hns2 sequence obtained from strain 042 Δhns (pLGhns2) corresponded to the WT hns2 gene. In contrast, PCR amplification of the hns2 gene from strain 042 Δhns (pLGhns2*) generated two bands ( Supplementary Fig. S4A). The size of one of them corresponded to the hns2 gene (likely resulting from the amplification of the chromosomal copy). Sequencing of the higher molecular mass amplicon showed that an IS5 element is inserted in the coding sequence of the hns2* gene, thus disrupting the hns2 coding sequence ( Supplementary Fig. S4B). This explains why H-NS2 expression dictated by plasmid pLGhns2* does not restore the WT growth rate in strain 042 Δhns (pLGhns2*).

H-NS2 expression levels influence
To further confirm that expression of H-NS2 dictated by plasmid pLGhns2* can be unwanted under some circumstances, we transformed both plasmids in strain XL1blue, and amplified by PCR and sequenced the hns2 gene. Again, the hns2 sequence of plasmid pLGhns2 corresponded to WT hns2, and that from plasmid pLGhns2* was disrupted by an IS5 element. In this context it is worth mentioning here that, when cloning the hns2* gene in the pFZY1 plasmid for the hns2 transcriptional studies, an intermediate step previous to the transformation of the recombinant plasmid in strain 042 is to transform the construct in an intermediate E. coli host. We tried as intermediate hosts three different strains: DH5α, XL1Blue and MG1655. In the former two strains, it was impossible to recover the pFZY1 plasmid harboring the hns2* gene. All isolates contained plasmids with the WT gene (i.e., the C > T transition had reverted). However, the construct pFZY1hns2* was stable in strain MG1655, and we could hence isolate plasmid from this strain and transform in strain 042 for the transcriptional analysis.

Temperature and role of the H-NS and H-NS2 proteins modulating gene expression in strain 042.
Temperature-dependent regulation of gene expression is a hallmark of the H-NS protein 32 . We showed previously that, at 37 °C, H-NS2 participates in the regulation of the expression of a subset of the H-NS modulated genes, mainly HGT genes 28 . Taking into account that the relationship between increased H-NS2 levels and enhanced growth rate in the 042 Δhns mutant takes place at 25 °C, we decided to study the regulatory role of both proteins in strain 042 at this temperature. To that end, we used RNA-seq to obtain the transcriptomes of strains 042 WT, 042 Δhns and 042 Δhns2 at 25 °C. Supplementary figure S5A,B show the functional categories of up-and downregulated genes in strains Δhns and Δhns2 when compared to the WT strain. Pathogenesis and bacterial metabolism are the functional categories that include a significant percentage of the genes that are upregulated in both Δhns and Δhns2 mutants. Those most upregulated genes in the Δhns and Δhns2 mutants at low temperature were identified and compared with the previously identified upregulated genes when cultures were grown at 37°C 28 . Table 2A,B compare those most upregulated genes in the Δhns genetic background at 25 °C and 37 °C. Table 3A,B compare those most upregulated genes in the Δhns2 genetic background at these two temperatures. The impact of the growth temperature on the regulatory role of H-NS and H-NS2 proteins is different. For the Δhns mutant, it is apparent that the sets of upregulated genes at 25 °C and 37 °C are similar, although the silencing role of H-NS is much stronger at low than at high temperature (deregulated genes show a much higher foldchange at 25 °C than at 37 °C). In contrast, the effect of the hns2 allele at low temperature is different to the effect observed at high temperature. The upregulated genes at 37 °C in the Δhns2 mutant (which  We also assessed whether, at 25 °C, overexpression of H-NS2 can reduce expression of those genes that are upregulated in an H-NS mutant. To that end, we selected five genes that are overexpressed in a 042 Δhns mutant at 25 °C, but not in an hns2 mutant under the same culture conditions. We used qRT-PCR to quantitate transcription of these genes both in a 042 Δhns mutant derivative of strain 042 and in one of the 042 Δhns derivatives that contains the C > T transition in the hns2 promoter (Fig. 5). When compared to the expression observed in the 042 Δhns mutant, expression in strain 042 Δhns phns2* is significantly lower in four of all five genes studied.

Discussion
Based on the results of the approach designed in Salmonella to identify mutations that increase the growth rate of hns mutants 29 , we expected to identify amino acid substitutions either in the StpA or in the H-NS2 sequences that would increase the capacity of any of these protein to more efficiently replace the function of the H-NS protein in the E. coli strain 042. Nevertheless, this was not the case. Growth of the 042 Δhns mutant at 25 °C readily led to the isolation of mutants mapping in the promoter region of the hns2 gene. When growing at this temperature, the fact that the different Δhns subcultures exhibiting a growth rate close to that of the WT strain did not harbor mutations in the stpA gene but the same C > T transition in the promoter region of the hns2 gene shows that this latter mutation is a genetic change that occurs at a frequency that, when needed, allows mutants to be readily selected. This was also the case for the double stpA hns derivative of strain 042. Rather than accumulating mutations in the rpoS gene or suffering amplifications of chromosomal sequences as it was the case for the E. coli strain MG1655 30 , the above referred mutation in the hns2 promoter region was selected upon subculturing the strain in the lab.
The C > T transition in the hns2 promoter increasing the growth rate of the 042 Δhns mutant is likely due to the fact that the resulting mutant promoter is stronger than the WT promoter and dictates an increased H-NS2 expression. A thymine at position -7 in the hns2 promoter is highly conserved in the TATA box of E. coli promoters and hence it justifies the increased promoter strength. No other effects (i.e., an altered transcriptional start site of the hns2 gene or the generation of novel target sequences for transcriptional activators) could be observed.
H-NS2 expression is significantly lower than H-NS expression in the WT strain 042. H-NS represses either directly or indirectly H-NS2 expression 28 . Hence, expression levels of the H-NS2 protein that are higher than those of the WT strain can only be positively selected under some circumstances (i.e., H.NS depletion). In other conditions, abnormally high-level H-NS2 expression can be actually deleterious. Examples are E. coli strains DH5α and XL1Blue, in which transformation of plasmid pFZY1phns2* generates clones harboring the WT hns2 promoter (this, in turn, showing that the C > T transition can be reverted), or strains 042 Δhns and XL1blue harboring plasmid pLGhns2*, in which the hns2 gene is disrupted by the insertion of an IS element. This shows that there exists an expression range of H-NS2 which may be beneficial for strain 042 under different conditions but, beyond that range, the effect on cell fitness is detrimental. The analysis of the differential role of the H-NS2 protein at 25 °C and 37 °C also correlates H-NS2 concentration and cell physiology. H-NS2 represses the expression of a subset of the H-NS regulated genes at 37 °C, but not at 25 °C. At low temperature, H-NS2 expression drops 28 and its role modulating gene expression is reduced. Only few genes show significant foldchange values.  www.nature.com/scientificreports/ The comparative analysis of the global transcriptomes of strain 042 Δhns at 25 °C and 37 °C is in accordance with the observed different impact of the hns mutation on the strain 042 growth rate at both temperatures. The foldchange of H-NS silenced genes at 25 °C is several times higher than that observed at 37 °C. Therefore, a drastically altered expression of several genes in the hns mutant growing at 25 °C must significantly impact the cell physiology and the growth rate. As shown in this work, phns2* directed expression of H-NS2 reduces the overexpression of these genes in the hns mutant, which in turn must result in an increased growth rate. With respect to the H-NS2 protein, the fact that its expression is lower at 25 °C than at 37°C 28 is likely underlying the reduced regulatory role that H-NS2 shows at low temperature.
Full induction of H-NS/H-NS2 repressed genes at 37 °C in strain 042 must occur in response to environmental stimuli different to temperature. The likely scenario for several of the H-NS targeted genes is: (i) H-NS strongly represses them at low temperature; (ii) a temperature increase (i.e., transition from 25 °C to 37 °C) alleviates H-NS silencing, enabling a partial expression of these genes. At that temperature (37 °C), both H-NS and H-NS2 contribute to partial gene silencing, and (iii), in response to other stimuli (i.e., osmolarity, pH, anti-silencing factors), H-NS/H-NS2 silencing is completely alleviated.
From the previously published data 28 and the results presented here at least two functions can be attributed to the H-NS2 protein: to coregulate gene expression with H-NS mainly at temperatures within the host, and to compensate for reduced H-NS (or H-NS/StpA) levels under specific circumstances.
The physiological conditions requiring that H-NS2 compensates for reduced H-NS levels must not be restricted to the occurrence of spontaneous mutations in the hns gene. Incorporation of HGT DNA by bacterial cells may result in the resident H-NS protein being titrated out because of targeting incoming AT-rich stretches of HGT DNA. Under these conditions, an increase of H-NS2 expression can avoid fitness loss. As commented above, some plasmids such as pSF-R27 encode an hns orthologue, the sfh gene. It was shown that expression of the Sfh protein in cells harboring plasmid pSF-R27 provides a stealth function, avoiding the fact that plasmid incorporation reduces host fitness because of resident H-NS protein being titrated out 24 . This function can be www.nature.com/scientificreports/ also accomplished by the chromosomally encoded H-NS2 protein. Hence, strains that have incorporated the hns2 gene provide themselves with a powerful regulatory tool that helps H-NS function under different physiological conditions. In addition to the EAEC strain 042, the H-NS2 protein is expressed in several other pathogenic E. coli strains and other enterobacterial genera, such as Salmonella, Klebsiella, Serratia or Citrobacter. In E. coli, the vast majority of the strains carrying the hns2 gene correspond to extraintestinal isolates encoding multiple antibiotic resistance genes in their genomes, such as Escherichia coli strain 4/1-1, Escherichia coli strain K-15KW01 and Escherichia coli strain SaT040. From the EAEC strains whose genome sequence is known, strain 042 is the only one encoding the hns2 gene. This speaks for hns2 acquisition being a recent event in this strain, happening upon differentiation of the EAEC pathotype from other E. coli lineages, H-NS2 comodulates with H-NS several virulence genes in strain 042, including up to 80 pAA genes, which speaks for the relevant regulatory role that this H-NS paralogue plays in strain 042.

Methods
Bacterial strains, plasmids and growth conditions. All the bacterial strains and plasmids used in this work are listed in Supplementary Table S1. Oligonucleotides used in this work are listed in Supplementary  Table S2.

Genetic manipulations and plasmids construction.
Mutant derivatives lacking the hns paralogue genes in the EAEC strain 042 were obtained by the λ Red recombinant method previously described 33 . Briefly, the antibiotic resistance determinant of the plasmid pKD4 (kanamycin) was amplified using the corresponding oligonucleotides hns p1/hns p2, hns2 p1/hns2 p2 and stpA p1/stpA p2 for hns, hns2 and stpA genes respectively (Supplementary Table S2). The mutants were confirmed by PCR using the KT primer (located inside the kanamycin resistance) in combination with specific primers that hybridizes in the remaining gene sequence in the bacterial chromosome (hnsp1 up for hns, hns2p1 up for hns2 and stpA p1 up for stpA), respectively (Supplementary Table S2). When necessary, the antibiotic resistance determinant was eliminated by using the FLP/ FRT-mediated site-specific recombination method, as previously described 34 . The double mutants were obtained by combining a previous deletion with another deletion generated by insertion of another antibiotic resistance cassette.
Recombinational transfer of the Flag-epitope into the C-terminal end of the hns2 gene was achieved by following the methodology previously described 35 . The template vector coding for the Flag-epitope and Km r determinant used was pSUB11. The oligonucleotides used for the construction of the H-NS2 Flag-tagged derivative were hns23X p1 and hns23X p2 (Supplementary Table S2). The correct insertion of the Flag-tag was confirmed by PCR using the oligonucleotides hns2 p1 up/hns2 p2 down (Supplementary Table S2).
The hns2 gene of E. coli 042 with a point mutation on its own promoter (clone obtained in the directed evolution experiment) was cloned into the low copy number pLG338-30 plasmid. Oligonucleotides hns2pLG338 ECORI fw 5 and hns2pLG338 BAMHI rev3 (Supplementary Table S2) were used to amplify by PCR the hns2 gene using the Phusion Hot Start II DNA polymerase (Thermo Scientific) following the manufacture´s recommendations. The resulting PCR fragment was purified using the GeneJET PCR purification Kit (Thermo Scientific) and digested with EcoRI and BamHI restriction enzymes (Thermo Scientific). Ligation was performed with pLG338-30 plasmid digested with the same restriction enzymes and treated with alkaline phosphatase (FastAP, Thermo Scientific). The resulting recombinant plasmid pLGhns2* was transformed in E. coli MG1655 cells. Plasmid extraction was carried out from positive clones using GeneJET Plasmid Miniprep Kit (Thermo Scientific) and subsequently Sanger sequenced for confirmation of correct in-frame insertion of the hns2 gene using the primers pLG338 EB Fw and pLG338 EB Rv (Supplementary Table S2).
For construction of transcriptional lacZ fusions with the hns2 promoter, the hns2 promoter region from E. coli 042 was PCR amplified by using the Phusion Hot Start II DNA Polymerase (Thermo Scientific), following the manufacturer´s recommendations, using the primers hns2 promoter Fw EcoRI/hns2 promoter Rev BamHI (Supplementary Table S2) and using as a templates the E. coli 042 wild type strain and the spontaneous mutant E. coli 042 Δhns with the C > T transition generated in the directed evolution experiment. The resulting PCR fragments were purified by using the GeneJET PCR purification Kit (Thermo Scientific) and digested with EcoRI and HindIII restriction enzymes (Thermo Scientific). Ligation was performed in the low copy plasmid pFZY-1 digested with the same restriction enzymes and treated with alkaline phosphatase (FastAP, Thermo Scientific). The resulting plasmids pFZY1phns2 (wild type hns2 promoter) and pFZY1phns2* (hns2 promoter with the C > T change) were transformed in E. coli MG1655 cells. Plasmid DNA was extracted from the transformants and purified by using the GeneJET PCR purification Kit (Thermo Scientific) and Sanger sequenced for confirmation of the correct in-frame insertion of the hns2 promoter by using the primers pFZY-1 p1up-lacZ Rv (Supplementary Table S2).
To introduce plasmids in E. coli, bacterial cells were grown until an optical density at 600 nm (O.D 600nm ) of 0.6-0.8. Once cells arrived at this level of growth, they were washed several times with 10% glycerol at 4 °C, and the respective plasmids were introduced by electroporation using an Eppendorf gene pulser (Electroporator 2510). β-galactosidase assay. β-galactosidase activity assays were performed as described previously 37 . Student´s t-test was used to determine the statistical significance, and the values were obtained by using the GraphPad Prism 5 software. A P value of less than 0.05 was considered significant.

RNA-Seq.
RNA-seq experiments were performed as previously described 28 .
Isolation of RNA. For RNA isolation, bacterial cells were grown until OD 600 of 2.0. Then, 5 ml of cells were mixed with a 0.2 × volume of a stop solution (95% ethanol, 5% phenol), shaken and centrifuged during 10 min at 6.000 × g. Bacterial pellets were subsequently frozen at -80 °C until use. Total RNA was extracted from bacterial pellets using Tripure Isolation Reagent (Roche) according to the manufacturer's instructions. Potential traces of DNA were removed by digestion with AmbionDNase I (RNase-free) according to the manufacturer's instructions. RNA concentration and quality were measured using a Nano-Drop 1000 (Thermo Scientific).
5′ RACE (Rapid amplification of cDNA ends). 5´ RACE assays were performed for the determination of the 5´-mRNA transcript of hns2 gene from strains 042 WT strain and its Δhns and Δhns hns2* derivatives. The assays were carried out essentially as reported 38 , with minor modifications as described. The 5´ triphosphates were converted to monophosphates by treatment of 12 µg of total RNA with 25 units of tobacco acid pyrophosphatase (TAP, Epicentre), 1 × final concentration of TAP buffer plus 0.5 µl of RNase Inhibitor (Ambion) during 1 h at 37 °C. Control RNA was incubated under the same conditions in the absence of the TAP enzyme. Before P:C:I (water-saturated phenol, chloroform, isoamyl alcohol mixture, 25:24:1, v/v) extraction, 500 pmol of the RNA adapter oligonucleotide A3 (Supplementary Table S2) were added to both reactions. After P:C:I extraction, RNAs were ethanol precipitated in the presence of 0.3 M sodium acetate (pH 5.7). RNAs were dissolved in water, heat-denatured at 90 °C for 5 min, and then quick-chilled on ice. The A3 adapter was ligated at 17 °C for 16 h by using T4 RNA ligase (Thermo Scientific) plus RNase Inhibitor (Ambion) pre-mixed in a ratio of 9:1 (RNA ligase:RNase Inhibitor), T4 RNA ligase buffer (Thermo Scientific) and 10% of DMSO. RNAs ligated to A3 oligonucleotide were then P:C:I purified and ethanol-precipitated. RNAs were redissolved in water, and 5 µg were reverse transcribed by using random primers and the High-capacity cDNA Reverse Transcription Kit (Applied Biosystems) according to the manufacturer's instructions. Reverse transcription was performed in three cycles of: 10 min at 25 °C, 120 min at 37 °C and 5 min at 85 °C. The products of reverse transcription were amplified by using the DreamTaq Hot Start Green DNA Polymerase (Thermo Scientific). For each 50 µl of PCR reaction, 2 µl of cDNA were used together with 0.5 µM of the hns2 gene specific (hns2-RACE Rv) and adapter specific (B6) primers (Supplementary Table S2). PCR products were separated on 2% agarose gels, and the single-band amplicons were purified by using the GeneJET PCR purification Kit (Thermo Scientific) and cloned into pCR2.1TOPO (Invitrogen) vectors following the manufacture´s recommendations. White colonies were screened for the presence Scientific Reports | (2020) 10:18131 | https://doi.org/10.1038/s41598-020-75204-4 www.nature.com/scientificreports/ of inserts of appropriate size by colony PCR using M13 Fw and M13 Rv primers (Supplementary Table S2), and Sanger sequenced using the same M13 primers.

Quantitative reverse transcription-PCR (qRT-PCR).
The expression level of the hdeA, EC042_ RS01720, EC042_RS23490, slp and hcp genes was determined by using real-time quantitative PCR. Briefly, 1 μg of previously isolated total RNA was reverse transcribed to generate cDNA by using a High-capacity cDNA Reverse Transcription Kit (Applied Biosystems) according to the manufacturer's instructions. All samples within an experiment were reverse transcribed at the same time. The resulting cDNA was diluted (1:100) in nuclease-free water and stored in aliquots at -80 °C until used. As a control, parallel samples in which reverse transcriptase was omitted from the reaction mixture were run. Real-time PCR was carried out by using the Maxima SYBR green/ROX qPCR Master Mix (Thermo Scientific) and an ABI Prism 7700 sequence detection system (Applied Biosystems). Specific oligonucleotides complementary to the genes of interest were designed by using the Primer3 software (Supplementary Table S2). The relative quantification of gene expression of mutants versus the wild-type strain was performed using the comparative threshold cycle (CT) method 39 . The relative amount of target cDNA was normalized by using the gapA gene as an internal reference standard. Student´s t-test was used to determine the statistical significance, and the values were obtained by using the GraphPad Prism 5 software. A P value of less than 0.05 was considered significant.
Bioinformatics analysis. UniProt (https ://www.unipr ot.org) accession numbers of differentially expressed genes were used to annotate the Gene Ontology (GO) terms. For the grouping of genes differentially expressed by categories a Python script was programmed 40,41 . The analysis of the hns2 promoter prediction was performed using the BPROM software (https ://www.softb erry.com/berry .phtml ?topic =bprom &group =progr ams&subgr oup=gfind b).