Transcriptional responses of Escherichia coli during recovery from inorganic or organic mercury exposure

Abstract

Background

The protean chemical properties of mercury have long made it attractive for diverse applications, but its toxicity requires great care in its use, disposal, and recycling. Mercury occurs in multiple chemical forms, and the molecular basis for the distinct toxicity of its various forms is only partly understood. Global transcriptomics applied over time can reveal how a cell recognizes a toxicant and what cellular subsystems it marshals to repair and recover from the damage. The longitudinal effects on the transcriptome of exponential phase E. coli were compared during sub-acute exposure to mercuric chloride (HgCl₂) or to phenylmercuric acetate (PMA) using RNA-Seq.

Results

Differential gene expression revealed common and distinct responses to the mercurials throughout recovery. Cultures exhibited growth stasis immediately after each mercurial exposure but returned to normal growth more quickly after PMA exposure than after HgCl₂ exposure. Correspondingly, PMA rapidly elicited up-regulation of a large number of genes which continued for 30 min, whereas fewer genes were up-regulated early after HgCl₂ exposure only some of which overlapped with PMA up-regulated genes. By 60 min gene expression in PMA-exposed cells was almost indistinguishable from unexposed cells, but HgCl₂ exposed cells still had many differentially expressed genes. Relative expression of energy production and most metabolite uptake pathways declined with both compounds, but nearly all stress response systems were up-regulated by one or the other mercurial during recovery.

Conclusions

Sub-acute exposure influenced expression of ~45% of all genes with many distinct responses for each compound, reflecting differential biochemical damage by each mercurial and the corresponding resources available for repair. This study is the first global, high-resolution view of the transcriptional responses to any common toxicant in a prokaryotic model system from exposure to recovery of active growth. The responses provoked by these two mercurials in this model bacterium also provide insights about how higher organisms may respond to these ubiquitous metal toxicants.

Electronic supplementary material

The online version of this article (10.1186/s12864-017-4413-z) contains supplementary material, which is available to authorized users.

Background

The common metallic element mercury (Hg) has no beneficial biological function and its chemical similarities to essential transition metals such as zinc, copper, and iron make it highly toxic to all living systems. Global mercury emissions range from 6500 to 8500 Mg annually with estimates of half [1, 2] and even two-thirds [3] being anthropogenic and the rest from volcanism. Mercury exists in multiple chemical forms that are readily susceptible to abiotic and biotic inter-conversions [4]. Mercury occurs naturally as the insoluble HgS ore (cinnabar), as inorganic complexes of Hg⁺², Hg⁺¹, or (Hg₂)²⁺ of varying solubility depending on available ligands, and as organomercurials generated by microbial and anthropogenic processes.

Major sources of chronic mercury exposure in humans include dental amalgam fillings [5, 6], consumption of fish containing methylmercury [7], and artisanal gold mining operations [8]. Organomercurials, like phenylmercury, methylmercury, and merthiolate (ethylmercury) have historically been used in medical, industrial and agricultural applications as antimicrobial or fungicidal agents [9–11]. The toxic effects of mercury exposure in humans are associated with neurological, kidney, liver, gastrointestinal, and developmental disorders [9, 12–15].

Like other common electrophilic toxic metals such as arsenic, cadmium, and lead, there is no single biochemical target for mercury damage. Mercury has a strong affinity for sulfur and selenium [16, 17] and therefore targets the cellular thiol pool, composed of glutathione and cysteine thiol groups of proteins [9] and selenocysteine, a rare but critical amino acid in proteins involved in redox defense and thyroid function [18]. Depletion of the cellular thiol pool and disruption of the cellular membrane potential by mercury can induce oxidative stress and apoptosis pathways in mitochondria [19, 20]. However, there is no evidence that mercury itself undergoes Fenton-type chemistry to generate reactive oxygen species like iron and copper [21].

In earlier work we used global proteomics to identify stable mercury-protein binding sites in growing E. coli cells exposed to acute levels of organic or inorganic Hg [22]. We found cysteine sites in several hundred proteins, many highly conserved evolutionarily, that formed stable adducts with one or more of these mercurials, consequently disrupting many cellular processes such as iron homeostasis and the electrolyte balance [23]. Importantly, we found that organic and inorganic mercurials had distinct effects on these cellular processes and distinct protein structural preferences. Although the pathobiology of organic and inorganic mercurials has been known for decades to differ, with methyl- and ethyl-mercury recognized as neurotoxic and inorganic mercury as neurotoxic, nephrotoxic, hepatotoxic, and immunotoxic, no previous studies at that time had assessed the biochemical underpinnings of these distinctions on a global scale in any model system.

Motivated by our proteomics observations and by microarray data from C. elegans showing distinct transcriptional single end point response and toxicity for inorganic and organic mercurials [24], we applied RNA-Seq to examine the transcriptional effects of HgCl₂ and phenylmercuric acetate (PMA) exposure on E. coli K-12 MG1655 over time. This is the first study to examine the global transcriptional response to mercury exposure in a microorganism and the only study to compare directly the effects of different compounds over time through recovery. The changes in gene expression were idiosyncratic for each compound, confirming and extending the idea that the cell suffers overlapping but distinct biochemical damage and marshals both distinct and overlapping recovery processes in response to these chemically distinct mercurials. Although our work was in a bacterium, the high evolutionary conservation of many of the genes whose expression we identified as mercury-vulnerable offers insights for the toxicology of mercury compounds in higher organisms.

Methods

Cell cultures

For each biological RNA-Seq replicate E coli K-12 MG1655 was subcultured from cryostorage on Luria-Bertani (LB) agar overnight at 37 °C. A half-dozen well-isolated colonies were used to inoculate a 20 ml starter culture in Neidhardt MOPS Minimal Medium (NM3) [25] (0.2% final glucose concentration) supplemented with 20 mg/L uracil and 500 μg/L thiamine, which was incubated at 37°C with shaking at 250 rpm overnight (~18 h). The overnight starter culture was diluted 1:30 to initiate the experimental culture and divided into three 500 ml flasks with 100 ml NM3 in each, which were incubated at 37°C with shaking at 250 rpm. When cultures reached OD₅₉₅ ≈ 0.470 (~ 200 min), two cultures were made 3 μM mercuric chloride (HgCl₂) or 3 μM phenylmercuric acetate (PMA) and the third was left as an unexposed control. Mercury stocks were prepared fresh for each growth experiment: 10 mM HgCl₂ (Fisher) in water and 5 mM PMA (Sigma) in 25% dimethyl sulfoxide DMSO (Fisher), which is 2.1 mM or 0.015% v/v final concentration DMSO in culture. These mercurial exposures were chosen from prior pilot experiments to find exposure conditions (OD₅₉₅, mercurial concentration and sampling times) that displayed a marked decrease in growth rate relative to the unexposed control but allowed subsequent restoration of rapid growth rate (i.e. recovery) within 1 h (approximately one generation in NM3) after mercurial exposure. Duplicate 1-ml aliquots of each culture were collected at 0 (unexposed control only), 10, 30, 60 min after mercurial exposure and immediately centrifuged at 20,800 x g for 3 min at 4 °C. Spent medium was aspirated and cell pellets were frozen at −70 °C within 5 min after collection. Seven biological replicates were prepared following this protocol and the average variance for all replicates in culture optical density over each 90-min experiment ranged from 0.0019 – 0.0073. The three biological replicates with the lowest variance between growth curves (range from 0.0007 – 0.0017 for all time points) were prepared for RNA-Seq.

Purification of mRNA

One cell pellet from each condition and sampling time was thawed on ice for all three biological replicates; total RNA was isolated by RNAsnap™ [26] and stored at −70 °C. DNA contamination was removed by two treatments with Turbo-DNase (Ambion; Life Technologies). RNA concentrations and A₂₆₀/A₂₈₀ ratios were determined using a Nanodrop™ 1000 spectrophotometer (Thermo Scientific). Ribosomal RNA depletion was performed with the Ribo-Zero™ rRNA removal kit for Gram-negative bacteria (Epicentre) and concentrated using RNA Clean and Concentrator™ -5 columns (Zymo Research) following the manufacturer’s instructions. Purified mRNA was quantified using the Nanodrop™ and stored at −70 °C.

Library preparation and next-generation sequencing

The quality and quantity of rRNA-depleted RNA was assessed on a 2100 Bioanalyzer RNA pico chip (Agilent Technologies) using the manufacturer’s recommendations. Next-generation sequencing (NGS) libraries were prepared using the Kapa biosystems NGS stranded library prep kit for RNA-Seq with dual indexed Illumina adapters. Library insert size was ~150 bp, as determined by high-sensitivity NGS fragment analysis kit for Fragment Analyzer™ (Advanced Analytical Technologies) using the manufacturer’s instructions. Quantification of each library was done by qPCR and all 30 libraries were pooled in equal concentrations. The library preparation, quality analysis, and pooling were performed by the Georgia Genomics Facility (http://dna.uga.edu). Paired-end (2 × 50 bp) sequencing of the pooled libraries using the Illumina HiSeq 2000 platform was performed by the HudsonAlpha Institute for Biotechnology Genomic Services Laboratory (http://gsl.hudsonalpha.org). See Additional file 1: Table S1 for index and filename information for data uploaded to NCBI Gene Expression Omnibus database (http://www.ncbi.nlm.nih.gov/geo/) with accession ID: GSE95575.

Data processing and differential expression analysis

Quality control processing of sequence data was performed using Galaxy (https://galaxyproject.org) on the Georgia Advanced Computing Resource Center at the University of Georgia. The FASTX tools in Galaxy (http://hannonlab.cshl.edu/fastx_toolkit) were used for filtering by quality (80% of sequence ≥ quality score of 20), then reads were trimmed at both 5′ and 3′ ends using a window and step size of 1 with quality score ≥ 20. Forward- and reverse-read mate-pairs were assembled and aligned to the Escherichia coli MG1655 K-12 genome using Bowtie2 [27]. SAMtools [28] was used to convert Bowtie2 output (.bam file) to SAM format. The number of sequence reads that aligned to features in the annotation file (Escherichia_coli_str_k_12_substr_mg1655.GCA_000005845.2.24.gtf from http://bacteria.ensembl.org) were tabulated from the resulting SAM alignment files using the HTSeq-count program [29] with intersection non-empty mode. Mapped read counts were analyzed for significant differential expression (false discovery rate of ≤0.01, fold-change ≥2) using the baySeq package in R [30]. All genes that did not meet both the ≤1% FDR and ≥2 fold-change criteria were indicated as no-change in figures, tables, and text. Within baySeq, two-way comparisons using quantile normalization were made for all three biological replicate transcriptomes over time for HgCl₂ exposure or PMA exposure versus the unexposed control. We also examined changes over time in the unexposed control culture itself.

Results

Effects of sub-acute mercury exposure on growth of MG1655

We defined sub-acute exposure as the concentration of mercury that clearly inhibited growth relative to the unexposed control but allowed cells to resume growth within 1 h or approximately one generation in this medium (Fig. 1a, Additional file 1: Figure S1). We chose restoration of growth rate, not stationary phase cell density, as the benchmark for recovery so as not to conflate normal cellular stationary phase “stop growing” signals with mercury-induced “stop growing” signals. Based on pilot experiments the appropriate dose proved to be 3 μM for both mercurials. Exposure to 4 - 5 μM HgCl₂ prevented growth resumption during 1 h and the effects of PMA exposure were similar at 3 and 5 μM; exposure to 2.5 μM of either mercurial did not consistently retard growth (data not shown).

Fig. 1.

Effects of sub-acute mercury exposure on growth of MG1655. a E. coli K12 MG1655 grown in MOPS minimal medium, unexposed (blue) or exposed to 3 μM HgCl₂ (red) or 3 μM PMA (green) during mid-log phase. Asterisks indicate sampling times for RNA-seq. Error bars are standard error (SEM) of 3 biological replicates for each culture condition. See Additional file 1: Figure S1 for full growth curve. b Significantly differentially expressed genes (DEG) counts (up-regulated or down-regulated) for HgCl₂ and PMA relative to unexposed control culture at each time point

Cell-associated Hg (Additional file 1: Table S2 and Supporting Information Methods) declined slowly as has been reported previously for low level HgCl₂ exposure of Hg sensitive cells and was attributed to non-specific endogenous reductants [31–33]. Bound Hg in cells exposed either to HgCl₂ or to PMA declined similarly from ~50% of total Hg added to culture at 10 min to ~20% at 30 min, after which Hg loss from PMA-exposed cells continued to decline to 11% of input at 60 min. In contrast, cell-associated Hg in cells exposed to HgCl₂ increased from 24% at 30 to 47% at 60 min. Presently, we have no simple explanation for this unexpected difference in cell-bound Hg in late exponential phase cultures, however it does echo our finding that cultures acutely exposed to 40 μM or 80 μM PMA or HgCl₂ bound 24% or 208% more Hg(II) than PhHg, respectively [23]. Also notable was a brief drop in the culture optical density immediately after PMA exposure consistent with some cell lysis as has been reported [34]. The lack of apparent lysis after divalent HgCl₂ exposure may be due to its ability to cross-link cell envelope proteins via their cysteines, which is not possible for monovalent PMA.

Transcriptome benchmarks

Paired-end libraries averaged over 9.5 million reads and mapped reads provided an average of 143X coverage (Additional file 1: Figure S2). The sequencing data were of high quality, requiring removal of only 11% as low-quality reads. Of the high-quality reads, 97% of reads mate-paired, 99.4% of paired reads mapped to the genome and 82% of reads mapped to an annotated genome feature on average from all libraries.

Overall 89% of annotated mapped reads were to coding regions (CDS) based on raw un-normalized read counts per gene output from HTseq-count program [29] (Additional file 1: Figure S3, Table S3 and Additional file 2: Table S4). Pearson correlations of raw read counts confirmed that no strong biases were introduced in biological replicates for each condition (Additional file 1: Figures S4-S6). That dispersion is slightly greater in both mercury exposure conditions than in unexposed cultures, especially at later time points, is consistent with perturbations of multiple cellular processes.

Mapped reads to rRNA constituted only 0.3% of total reads (std. dev. = 0.425) on average for all libraries (Additional file 1: Table S3) consistent with effective Ribo-Zero™ rRNA removal. In the unexposed culture non-coding RNA’s (ncRNA) were 4% of total reads over all time points, but their percentage increased in mercury exposure conditions indicating greater differential expression of some ncRNA genes (details below). The very abundant tmRNA (ssrA) needed for rescuing stalled ribosomes [35] was 6% of total reads in the unexposed condition and although this percentage increased for mercury exposure conditions, the tmRNA gene (ssrA) was not differentially expressed under any condition. Pseudogenes accounted for less than 1% of total reads, but up to 35% (HgCl₂) and 13% (PMA) of them were significantly up-regulated. The tRNA’s were less than 1% of total reads because the library preparation method we used was not optimized for such small RNAs. However, approximately 35% of these observed tRNA genes were significantly down-regulated during the first 30 min after exposure to either mercurial.

HgCl₂ and PMA transcriptional responses are not the same

We expected that significantly differentially expressed genes (DEGs) in the mercury exposure conditions (compared to the unexposed cells) would change over time as the cells transitioned from initial growth stasis back into a normal growth rate. We also expected that some DEG responses would be similar because both mercurials are thiophilic and will bind to the cellular thiol redox buffer, glutathione (GSH), and to protein cysteine residues. However, since there are physiological differences and protein site preferences for each compound in acute Hg(II)- or PMA-exposure [23 and Zink et al. in preparation] we aimed here at a low exposure using a longitudinal protocol to discern more subtle distinctions between these mercurials as the cells experienced stasis and then recovered their growth rate. In the following sections, we first describe the bulk measures of gene expression over time and then describe differences in specific functional pathways.

Differentially expressed genes: the view from 30,000 ft

Differentially expressed genes (DEG) for each condition and time point

DEGs were determined by pairwise comparisons of mercury exposure conditions relative to the unexposed culture at the corresponding time point (Fig. 1b and Additional file 3: Table S5). Ten minutes after exposure, expression of 41% or 49% of the 4472 non-rRNA genes changed significantly for HgCl₂ or PMA-exposed cells, respectively (Fig. 1b). At 30 min with growth still arrested, 32% of genes in the HgCl₂-exposed cells were differentially expressed (Fig. 1b, a red). In contrast, PMA-exposed cells at 30 min began to recover their prior growth rate (Fig. 1a, green), but 45% of their genes remained differentially expressed (Fig. 1b). By 60 min, the PMA-exposed cells were growing at nearly their pre-exposure rate and only 1.5% of genes were differentially expressed, whereas the HgCl₂-exposed cells were still growing more slowly than pre-exposure with 13% of their genes still differentially expressed compared to the unexposed cells (Fig. 1b).

Shared and unique genes at each time point for each exposure

The total distinct DEGs across all time points was slightly lower for HgCl₂ (2327) than for PMA (2541) exposure (Fig. 1b and Additional file 1: Figure S7). More striking were the differences in DEGs at each time point; PMA-exposed cells modulated 20% more genes at 10 min (2181 vs 1821) and 40% more at 30 min (2007 vs 1422) than HgCl₂ exposed cells. This trend completely reversed by 60 min when DEGs declined in both exposure conditions but HgCl₂ exposed cells were still modulating ~9-fold more genes (563) than PMA-exposed cells (65), consistent with the latter recovering normal growth sooner (Fig. 1a). Also notable is the carryover of DEGs from one time point to the next where HgCl₂ exposed cells have 1001 DEGs in common at 10 and 30 min after exposure but that number is 65% greater in PMA-exposed cells (1650) (Additional file 1: Figure S7). However, HgCl₂ exposed cells have 52% more DEGs that are unique at 10 min compared to PMA-exposed cells (804 vs 529), i.e. more HgCl₂ provoked DEGs occur sooner after exposure than later. HgCl₂ exposure also yields more DEGs that occur at all time points compared to PMA (Additional file 1: Figure S7) since there are very few DEGs at 60 min for PMA exposure.

Up-regulated vs. down-regulated genes for each exposure

Sorting expression simply into genes up-regulated or down-regulated by HgCl₂ or PMA at each time point (Fig. 2) revealed additional quantitative distinctions between them. For up-regulated genes, PMA-provoked more unique DEGs than DEGs in common with HgCl₂ exposure at all time points, in contrast to HgCl₂ which had more DEGs in common than unique at all but the last time point. This trend was not continued for down-regulated genes where more genes were in common for both compounds than unique at all time points.

Fig. 2.

Overlap between differentially expressed genes at each sampling time. The 3 μM HgCl₂ exposure is in red and the 3 μM PMA exposure in green. Ovals are to scale only at each time point, but not between between time points in a panel nor between left and right panels

Thus, early in exposure the cell reduced expression of a similar number of genes for both mercurials, but up-regulated expression of many more genes in response to PMA than to HgCl₂, and these distinct trends persisted to the middle time point. By 60 min, gene expression of PMA-exposed cells closely resembled that of unexposed cells, but HgCl₂ exposed cells still have many up- and down-DEGs, consistent with slower growth rate recovery by HgCl₂ exposed compared to PMA-exposed cells (Fig. 1a).

Differentially expressed genes grouped by functional category

To sort our observations from a different perspective, the DEGs for each condition were grouped by Clusters of Orthologous Groups (COGs) to identify expression differences based on gene functions (Fig. 3 and Additional file 4: Table S6). For most COGs, both mercurials elicited their strongest responses, up- or down-regulated, within the first 10 min of exposure (Fig. 3); in most cases, the responses were of similar magnitude. At 30 min, the PMA (green) responses remained nearly the same, up- or down-regulated, but HgCl₂ provoked responses (red) generally diminished, often sharply. By 60 min, expression in PMA-exposed cells was barely distinguishable from the unexposed cells in all COG categories, whereas HgCl₂ exposed cells had notable differential expression in most COG categories.

Fig. 3.

Counts of differentially expressed genes for each condition grouped by COG functional category. Genes with a log₂ fold-change ≥1 for each condition were grouped by COG group. Positive counts represent observed up-regulated genes and negative counts represent observed down-regulated genes. COG code, number of proteins encoded by genome and category description: (A, 2) RNA processing and modification; (C, 284) Energy production and conversion; (D, 39) Cell cycle control, cell division, chromosome partitioning; (E, 355) Amino acid transport and metabolism; (F, 107) Nucleotide transport and metabolism; (G, 381) Carbohydrate transport and metabolism; (H, 179) Coenzyme transport and metabolism; (I, 121) Lipid transport and metabolism; (J, 236) Translation, ribosomal structure and biogenesis; (K, 294) Transcription; (L, 139) Replication, recombination and repair; (M, 242) Cell wall, membrane and envelope biogenesis; (N, 102) Cell motility; (O, 156) Post-translational modification, protein turnover, chaperones; (P, 223) Inorganic ion transport and metabolism; (Q, 68) Secondary metabolites biosynthesis, transport and catabolism; (R, 261) General function prediction only; (S, 203) Function unknown; (T, 191) Signal transduction mechanisms; (U, 50) Intracellular trafficking, secretion, and vesicular transport; (V, 91) Defense mechanisms; (W, 31) Extracellular structures; (X, 60) Mobilome, prophages, transposons

The four well-defined COG categories with the most DEGs were energy production (C), amino acid metabolism (E), carbohydrate metabolism (G), and transcription (K), which are also categories with a large number of genes (284, 355, 381, and 294 respectively) in E. coli (Fig. 3 legend). COG categories R and S encoding poorly defined (261) or non-defined (203) genes were also represented proportionally. These data suggest both mercurials broadly affect most metabolic categories, albeit to different degrees and at different rates. However, four well-defined COG categories have strikingly different responses to HgCl₂ and PMA. COG categories for nucleotide metabolism (F), translation (J), motility (N), and intracellular trafficking (U) have many fewer up-regulated genes in HgCl₂ exposed cells than in PMA-exposed cells. There are relatively few DEGs involved in cell division (D), extracellular structures (W), and mobile genetic elements (X) and genes within these categories responded similarly to both mercurials. Thus, grouping DEGs by COGs illuminates the broad functional differences and similarities between HgCl₂ and PMA exposure. Moreover, this view makes clear that DEGs occur in all functional categories for both compounds, but still display distinct differences in global transcriptional response to each compound. We provide gene-level detail on several of these functional groups below. Note that the COG database only includes functional annotations for 3398 of E. coli’s 4497 genes, but functional categories discussed below in more detail are not limited to COG-annotated genes.

A heat map of the DEGs log-fold changes (Fig. 4) provides a more granular look at all DEGs for both compounds across all time points. The heat map, using Ward’s minimum variance clustering method [36], shows considerable uniformity of up- and down-regulated expression during the 30 min after PMA exposure. In contrast, although HgCl₂ exposed cells grossly shared many DEGs with PMA-exposed cells (Fig. 2), the heat map reveals a more variegated response to Hg(II) in which different genes are up- or down-regulated at all time points, in contrast to the relatively consistent response of PMA during recovery. Overall, 34% of DEGs are unique to only one mercurial and ~3% of all DEGs had an opposite response to each compound (Additional file 3: Table S5). The most dramatic differences were at 60 min when HgCl₂ exposed cells were still modulating many genes but PMA-exposed cells had only minor differences with unexposed cells, consistent with their faster recovery of normal growth (Fig. 1a). We dissect some of these differences in function-specific heat maps below.

Fig. 4.

Differentially expressed genes at each RNA sampling time. Heat map of all genes that were differentially expressed in at least one mercury exposure condition (n = 3149). Genes were clustered by row using Ward’s minimum variance method [36] with non-squared log₂ fold-change input values

We also used STRING (version 10.0) [37, 38] for unsupervised network analysis to identify gene clusters that were up-regulated in response to each compound (Additional file 1: Figure S8 and Additional file 5: Table S7). We focused on up-regulated genes on the working assumption that they are more likely to contribute to recovery than genes whose expression is turned down. Gene clusters were generated by STRING based on organism specific data mining to identify genes with a functional association, such as a common biological purpose, location within the same operon, or shared regulatory mechanism. Note that this network algorithm does not consider fold-change intensity of response; it enumerates only whether an up-regulated gene is present at a given time point. The up-regulated DEGs (nodes) of HgCl₂ exposed cells formed several tight clusters encompassing 16 gene-ontology functions (GOFs) at 10 min, nine GOFs at 30 min, and seven GOFs at 60 min (Additional file 1: Figure S8 and Additional file 5: Table S7). In contrast, although there were more nodes for PMA-exposure at 10 and 30 min, there were fewer edges yielding no well-defined clusters at 10 min and only two GOFs at 30 min. This network analysis suggests that, although PMA provokes more DEGs than Hg(II) does, there is less functional congruence between the genes involved in the response to PMA. Specific gene and function changes are discussed further in the next section.

Lastly, as a control for using RNA-Seq in a longitudinal experiment, we observed DEGs at sequential time points in the unexposed control culture (Additional file 1: Figure S9 and Additional file 6: Table S8). As expected, changes were gradual over time with no more than 5% of the genome being differentially expressed from one time point to the next. At the 60 min time point, as the cells approached stationary phase 815 genes were differentially expressed compared to mid-log (time 0). Sorting these DEGs by COGs (Additional file 1: Figure S9) and by STRING network analysis (Additional file 1: Figure S10 and Additional file 5: Table S7) showed, as expected, many DEGs were consistent with normal transitioning from mid-log to late-log phase [39, 40].

Higher resolution view of expression differences in specific functional groups during recovery from exposure to HgCl₂ or PMA

Taking the perspective that a toxicant is a kind of signaling molecule, we considered differences in gene expression for the 2 Hg compounds to reflect how the cell senses the biochemically distinct damage produced by these two metallo-electrophiles as manifest by what tools the cell calls upon to restore its viability. A quick snapshot of the great extent of these compound-specific differences can be seen in the genes with a > 20-fold increase in differential expression after HgCl₂ exposure (Table 1) or PMA exposure (Table 2). Here we emphasize up-regulated genes on the working assumption they could contribute directly or indirectly to repairing damage caused by mercurial exposure. The 25 genes highly up-regulated by HgCl₂ (Table 1) are involved in altering the cell surface, oxidative stress response and repair, protein chaperones, metals homeostasis, and ribonucleotide reductase. The vestigial prophage genes likely play no rescue role for the cell and were simply activated by generalized stress responses and have large fold-change values due to repressed expression under normal growth conditions. The corresponding PMA response echoed only 8 of these 25 HgCl₂ high-responders, and notably did not include the vestigial phage genes.

Table 1.

Genes with ≥20 fold-change for at least two time points after HgCl₂ exposure (n = 25)

Gene ID	Gene Name	Product Description	Hg t10	Hg t30	Hg t60	PMA t10	PMA t30	PMA t60
b1112	bhsA	Biofilm, cell surface and signaling defects, YhcN family	1949	563	94	46	21	n.s.
b4458	oxyS	OxyS sRNA activates genes that detoxify oxidative damage	1524	1292	150	10	6	n.s.
b4249	bdcA	c-di-GMP-binding biofilm dispersal mediator protein	596	79	7	16	2	n.s.
b3686	ibpB	Chaperone, heat-inducible protein of HSP20 family	402	124	281	37	211	9
b0812	dps	Stress-induced Fe-binding and storage protein	339	52	n.s.	4	2	n.s.
b4248	yjgH	Putative reactive intermediate deaminase, UPF0076 family	296	24	3	6	2	n.s.
b0849	grxA	Glutaredoxin 1	246	33	n.s.	14	4	n.s.
b1144	ymfJ	Function unknown, e14 prophage	185	39	n.s.	3	3	n.s.
b2582	trxC	Thioredoxin 2, zinc-binding; Trx2	134	50	7	24	24	n.s.
b1147	ymfL*	Function unknown, e14 prophage	95	29	n.s.	n.s.	3	n.s.
b1146	croE*	Cro-like repressor, e14 prophage	90	40	n.s.	n.s.	n.s.	n.s.
b3687	ibpA	Chaperone, heat-inducible protein of HSP20 family	86	19	41	10	28	4
b2531	iscR	Transcriptional repressor for isc operon; contains Fe-S cluster	62	48	9	12	18	n.s.
b1148	ymfM*	Function unknown, e14 prophage	49	21	n.s.	n.s.	n.s.	n.s.
b4599	yneM	function unknown, membrane-associated; regulated by PhoPQ	38	36	n.s.	3	3	n.s.
b2673	nrdH	NrdH-redoxin reducing oxidized NrdEF	35	127	21	7	14	n.s.
b4030	psiE	Pho regulon, regulated by phoB and cAMP	35	64	17	38	59	n.s.
b1684	sufA	Scaffold protein for assembly of iron-sulfur clusters	32	39	5	n.s.	3	n.s.
b1748	astC	Succinylornithine transaminase; carbon starvation protein	30	31	25	34	36	n.s.
b4663	azuC	Function unknown; membrane-associated	27	25	36	41	49	n.s.
b0484	copA	Copper-, silver-translocating P-type ATPase efflux pump	25	20	n.s.	5	n.s.	−10
b2674	nrdI	Flavodoxin required for NrdEF cluster assembly	21	73	22	4	7	n.s.
b1747	astA*	Arginine succinyltransferase, arginine catabolism	10	20	29	9	14	n.s.
b1020	phoH	ATP-binding protein, function unknown	8	71	221	61	365	n.s.
b4002	zraP	Zn-dependent periplasmic chaperone	3	27	43	n.s.	n.s.	−3

Table is sorted by Hg at 10 min column. n.s. = not significantly different from unexposed culture and boldface highlights actual values ≥20-fold. Gene names in boldface have a ≥ 20 differential expression response to both Hg and PMA in at least one time point (n = 8). Genes marked with an asterisk (*) had fewer than 11 average read counts for at least 2 time points in the unexposed condition and were operationally defined as being “off” in that condition. Such genes constituted, the lowest 15th percentile of all genes, based on raw read counts normalized across all libraries and across all biological replicates

Table 2.

Genes with ≥20 fold-change in at least two time points for PMA exposure (n = 17)

Gene ID	Gene Name	Product Description	Hg t10	Hg t30	Hg t60	PMA t10	PMA t30	PMA t60
b3728	pstS	ABC phosphate transport system; periplasmic binding protein	n.s.	16	8	86	165	n.s.
b1020	phoH	ATP-binding protein, function unknown	8	71	221	61	365	n.s.
b0996	torC*	c-Type cytochrome	n.s.	n.s.	n.s.	55	65	77
b4060	yjcB	Function unknown	33	11	12	52	35	n.s.
b0399	phoB	Positive response regulator for pho regulon	4	22	3	51	105	n.s.
b1530	marR	Transcription repressor of multiple antibiotic resistance	26	7	n.s.	48	29	n.s.
b1531	marA	Transcriptional activator for multiple antibiotic resistance;	15	9	n.s.	46	31	n.s.
b1112	bhsA	Biofilm, cell surface and signaling defects, YhcN family	1949	563	94	46	21	n.s.
b1532	marB	marRAB multiple antibiotic resistance operon	16	8	n.s.	45	27	n.s.
b4663	azuC	Function unknown; membrane-associated	27	25	36	41	49	n.s.
b4030	psiE	Pho regulon, regulated by phoB and cAMP	35	64	17	38	59	n.s.
b3686	ibpB	Chaperone, heat-inducible protein of HSP20 family	402	124	281	37	211	9
b1748	astC	Succinylornithine transaminase; carbon starvation protein	30	31	25	34	36	n.s.
b3469	zntA	Zn(II), Cd(II), and Pb(II) translocating P-type ATPase	40	19	8	29	22	n.s.
b2582	trxC	Thioredoxin 2, zinc-binding; Trx2	134	50	7	24	24	n.s.
b4354	yjiY	Predicted transporter, function unknown	n.s.	n.s.	n.s.	20	77	n.s.
b1625	cnu	OriC-binding complex H-NS/Cnu	n.s.	10	n.s.	20	24	n.s.

Table is sorted by PMA at 10 min column. n.s. = not significantly different from unexposed culture and boldface highlights actual values ≥20-fold. Gene names in boldface have a ≥ 20 differential expression response to both Hg and PMA in at least one time point (n = 11). Genes marked with an asterisk (*) had fewer than 11 average read counts for at least 2 time points in the unexposed condition and were operationally defined as being “off” in that condition. Such genes constituted, the lowest 15th percentile of all genes, based on raw read counts normalized across all libraries and across all biological replicates

For PMA, the highly up-regulated genes are a distinct contrast to those for HgCl₂. First, the maximum amplitude of the PMA-provoked differential expression is generally much less than for Hg(II)-provoked high differential expression (Table 1), which could reflect the lower uptake of PMA. Secondly, while 11 of the 17 PMA-provoked genes were also on the HgCl₂ highly differential expression list, ion transport and antibiotic resistance loci were more prominent with PMA and prophage genes were absent.

These two snapshot tables make the points that both mercurials generate broad, but idiosyncratic, cellular responses. To place these “tips of many icebergs” in their larger cellular context, we used heat maps and tables of subsets of functionally related genes to discuss the differential effects of HgCl₂ and PMA on 12 canonical cellular systems in the following sections.

Informational macromolecules

DNA replication, recombination and repair

Of the 24 genes for initiation and maintenance, and termination of chromosome replication, there were more genes down-regulated (8) than up-regulated (3) in response to HgCl₂ and an equal number up- or down-regulated genes (7) in response to PMA (Additional file 7: Table S9). Of the 14 genes encoding the replicative polymerase holoenzyme, four genes capable of translesion synthesis (polB, dinB, umuCD) were up-regulated more by HgCl₂ exposure (Additional file 7: Table S9), suggesting a greater degree of direct or indirect DNA damage by HgCl₂ exposure. Of the 45 genes for repair and recombination proteins the transcriptional response to each mercurial was very similar (11 up-regulated and 16 down-regulated for HgCl₂; 9 up-regulated and 18 down-regulated for PMA). But there were repair genes unique to each compound: xthA, uvrAB, mutM, and recN were only up-regulated by HgCl₂; and mutH and mutY were only up-regulated by PMA.

The recA, recN, and xthA DNA repair genes were the most highly up-regulated (≥10 fold) in response only to HgCl₂. The recA gene, induced by double-strand DNA breaks, serves multiple roles in DNA repair [41, 42]. Curiously, expression of recBCD, which is needed for break repair, either did not change or declined compared to unexposed cells for both mercurials. Expression of several genes involved in repair (recG, nth, hsdS, and mcrC) were down-regulated by both compounds, but with larger negative fold-changes for PMA than HgCl₂. Thus, the cells responded quickly to both mercurials, but some distinct responses suggest these two compounds directly or indirectly yield different kinds of DNA damage.

Transcription

Of the core RNA polymerase (RNAP) genes only PMA-exposure increased expression of a single gene rpoZ (ω subunit), but expression decreased in the remaining rpoABC core genes (Additional file 8: Table S10). HgCl₂ exposure did not change expression of any RNAP core genes except for a transient 3-fold drop in rpoA at 30 min. Only one of the five termination factors, the Rho-directed anti-terminator, rof, increased and did so for both mercurials with PMA again provoking a greater response.

Genes for three sigma factors displayed increased expression upon exposure to either mercurial, with rpoH (heat shock sigma factor) and rpoS (stationary phase and stress response sigma factor) increasing more following PMA-exposure and rpoD (housekeeping sigma factor) only increasing after HgCl₂ exposure. The effects of HgCl₂ or PMA exposure on the regulation of genes within each regulon controlled by E. coli’s seven sigma factors are tabulated in Additional file 9: Table S11. Many genes are modulated differentially by HgCl₂ or PMA-exposure, but no single sigma factor is uniquely responsible for increases or decreases in responses to these two compounds.

Many of the 203 transcriptional regulators annotated in the RegulonDB (Table 3) [43, 44] and the 1723 genes they control were expressed differently with the two mercurials (Additional file 10: Table S12). PMA provoked up-regulation of more transcription factor genes at 10 and 30 min than HgCl₂ exposure, but slightly fewer down-regulated regulators (Table 3). Of all COG categories, transcription had the most up-regulated genes for both mercurials (Fig. 3 and Additional file 4: Table S6). PMA up-regulated ~40% more transcription related genes at 10 min and ~80% more genes at 30 min than HgCl₂. Six activators (mhpR, glcC, gadX, soxS, mlrA, phoB) and three repressors (mcbR, iscR, betI) were up-regulated at all times for HgCl₂, but gadX was the only activator gene up-regulated at all times for both mercurials (Additional file 10: Table S12). GadX is part of the RpoS regulon [45] and activates the acid resistance system and multidrug efflux [46, 47]. Details of transcription factors and their regulons are provided in Additional file 10: Table S12.

Table 3.

Changes in transcription factor gene expression

Transcription factors (n = 203)
	Hg_t10	Hg_t30	Hg_t60	PMA_t10	PMA_t30	PMA_t60
Up	63 (31)	46 (23)	14 (7)	86 (42)	78 (38)	1 (0.5)
Down	28 (14)	28 (14)	13 (6)	22 (11)	23 (11)	2 (1)

The sum of transcription factor genes either up-regulated or down-regulated is shown with the percentage of the total transcription factor genes in parenthesis; percents do not total 100 because genes with no change compared to unexposed cells are not tabulated here. See details in Additional file 10: Table S12

Lastly, E. coli has 65 currently annotated (ASM584v2), small non-coding RNAs. Although our RNA purification and library preparation methods were not optimized for their enrichment, we observed differential expression for a number of them (Additional file 3: Table S5, feature type “ncRNA”). ncRNAs up-regulated for both mercurials are involved in regulation of acid resistance (gadY), oxidative stress (oxyS), and multiple transporters (gcvB and sgrS). In contrast, adhesion and motility (cyaR), and anaerobic metabolism shift (fnrS) were down-regulated by both compounds.

Translation

Upon HgCl₂ exposure 83 and 74% of ribosomal proteins (r-proteins) were down-regulated at 10 and 30 min, respectively, versus only 4 and 41% for PMA at the corresponding times (Fig. 5 and Additional file 1: Figure S9; data for all functional group heat maps are shown in Additional file 11: Tables S13 and Additional file 12: Table S14). Transcription of r-proteins is repressed directly by binding of the nutritional stress-induced nucleotide ppGpp and DksA protein to RNAP [48]. The ppGpp synthase genes, spoT and relA, were down-regulated or unchanged, but expression of dksA was up-regulated for both HgCl₂ and PMA exposure. R-protein expression can also be inhibited by excess r-proteins binding to and inhibiting translation of their own mRNAs [49, 50].

Fig. 5.

Ribosomal subunit protein genes. Genes are grouped and colored by operon (see larger Additional file 1: Figure S11 and Additional file 11: Table S13 for details)

Translation initiation and elongation factors were largely unchanged, but expression of all three peptide chain release factor genes were down-regulated for PMA and the ribosome recycling factor (frr) was up-regulated only for PMA, consistent with interruption of translation. Eight tRNA-synthase genes declined with HgCl₂ but PMA caused only four tRNA-synthase genes to decline and two to increase in expression (Additional file 12: Table S14). Both mercurials caused a relative decline in tRNA expression for most amino acids, especially arginine, lysine, methionine, tyrosine, and valine tRNAs. With very few exceptions, ribosome assembly and translation were shut down for up to 30 min by both compounds, but returned to normal levels by 60 min.

Macromolecular turnover and chaperones

Divalent inorganic mercury can stably crosslink proteins and their subdomains via cysteines, disrupting 3-dimensional structures and allosteric movements [51–53]. Although monovalent PMA cannot cross-link, it forms a bulky adduct with cysteines [23], which may compromise protein folding. The proteases and chaperones of the heat shock response degrade or repair misfolded proteins [54] and we found their expression was increased by both mercurials (Fig. 6 and Additional file 1: Figure S12 and Additional file 11: Table S13). At 10 min, expression of protease genes lon, clpXP, and ftsH had risen 4- to 6-fold with HgCl₂ and lon and clpXP, but not ftsH, were up-regulated 3-fold with PMA. HgCl₂ provoked up-regulation of all 12 heat shock protein (HSP) and chaperone genes by 10 min, but only chaperones clpB and ybbN mRNAs remained elevated at 30 min. Two other HSP genes, Hsp15 (hslR) involved in stalled ribosome recycling and Hsp31 (hchA) an amino acid deglycase, were further up-regulated by HgCl₂ at 60 min. In contrast, at 10 min PMA had up-regulated only five HSPs, increasing to six by 30 min and declining to three by 60 min. The ibpA and ibpB chaperone genes were among the most highly up-regulated genes for both HgCl₂ and PMA and persisted throughout recovery.

Fig. 6.

Protein and RNA turnover and repair. (see larger Additional file 1: Figure S12 and Additional file 11: Table S13 for details)

Of the 16 RNases and RNA processing enzymes only 3 increased: RNase R (3-fold for HgCl₂ and 5-fold for PMA) for both compounds during first 30 min; RNase III two-fold for PMA at 30 min; and RNase T two-fold for HgCl₂ at 60 min. The degradasome complex subunit genes (rne, eno, rhlB, pnp, ppk) [55] were all down-regulated for PMA during the first 30 min following exposure, except the helicase (rhlB), but only enolase was down-regulated for HgCl₂ (Fig. 6 and Additional file 1: Figure S12 and Additional file 11: Table S13). Expression of RNase II (rnb) was also down-regulated for both compounds, but with relatively greater fold-changes observed for PMA. It is unclear what effect these changes in gene expression could have on RNA turnover and message decay rates while under mercury stress. As with the DNA metabolism genes, expression of the transcriptional apparatus shows that sufficient PMA was taken up to elicit both positive and negative responses distinct from HgCl₂.

Energy production

Electron transport chain

Expression of approximately 50% of all electron transport chain (ETC) genes was down-regulated during the first 30 min for HgCl₂ and PMA, with individual gene responses being very similar for both compounds (Fig. 7 and Additional file 1: Figure S13 and Additional file 11: Table S13). By 60 min, only 26% of these genes were down-regulated for HgCl_2, and none were down-regulated for PMA. Expression of NADH:unbiquinone oxidoreductase genes was down-regulated by both compounds, with 77 and 100% of these genes being down-regulated at 10 and 30 min, respectively. The ATP-synthase subunit genes were also strongly down-regulated by both mercurials at 10 and 30 min, but normal expression was restored at 60 min.

Fig. 7.

Electron transport chain and ATP-synthase. (see larger Additional file 1: Figure S13 and Additional file 11: Table S13 for details)

The torCAD locus that encodes the trimethylamine N-oxide anaerobic respiratory system was strongly up-regulated only by PMA exposure. This is likely an artifact of low-level basal expression and the dimethyl sulfoxide used to dissolve PMA. The final DMSO concentration, 0.015% vol/vol (2.1 mM), was not expected to have any biological effect [56] and the anaerobic DMSO reductase genes (dmsABC) were down-regulated. It is unlikely that either the tor or dms responses affect growth rate [57] or afford protection against either mercurial since over-expressed heme-dependent torC may be in the apoprotein form [58].

Carbon metabolism

Expression of genes for carbon metabolism decreased generally, but there were more up-regulated genes in response to HgCl₂ and not all steps were affected equally by both mercurials (Additional file 1: Figure S14). Expression of five genes of the pentose-phosphate pathway rose in at least one time point for HgCl₂, but only pgl increased for PMA at 10 min. The ribose-5-phosphate isomerase gene (rpiB), which is a backup enzyme for the gene product of rpiA [59], was up-regulated 40-fold for HgCl₂ at 10 min; although expression of rpiA did not differ from the unexposed cells for either mercurial at any time. Glycolysis responded similarly to both mercurials, with the greatest number of these genes being down-regulated at 30 min. The expression changes in TCA cycle genes were distinct for HgCl₂ and PMA; six genes were up-regulated in at least one time point for HgCl₂ and only one was up-regulated for PMA. Expression of several carbohydrate transport genes was down-regulated by both mercurials (Additional file 4: Table S6).

Nicotinamide adenine dinucleotide (NAD)

Expression of genes for nicotinamide adenine dinucleotide (NAD) and NAD-phosphate (NADP) synthesis and turnover pathways was repressed by mercury exposure (Additional file 1: Figure S15). The biosynthesis genes were moderately down-regulated, with nadB being the only gene down-regulated for both mercurials at all times and nadA decreasing for HgCl₂ at 30 and 60 min and for PMA at 30 min. Expression of the pncABC salvage pathway did not change. The NAD reduction pathways were more affected than the NADP reduction pathways, with only pgi down-regulated for both mercurials and edd down-regulated only for HgCl₂. The transhydrogenase (pntAB) was down-regulated only for PMA at 10 and 30 min. Expression of other genes for NAD to NADH reduction in glycolysis and the TCA cycle were also down-regulated for both mercurials, which reflects the overall decrease in metabolism and energy production pathways.

Globally, redox metabolism declined immediately after exposure and normal gene expression levels were not restored until growth recovered to the pre-exposure rate. KEGG maps created using iPath [60] depict system-wide metabolism changes over time (Additional file 1: Figures S16-S18 for HgCl₂ and Additional file 1: Figures S19-S21 for PMA).

Central metabolism

Amino acid metabolism and transport

The two mercurials had distinct effects on expression of genes for biosynthesis of amino acids (Fig. 8 and Additional file 1: Figure S22). Since mercury targets cysteine thiol groups and will deplete the cellular reduced thiol pool, we expected an increase in cysteine and glutathione biosynthesis. Surprisingly, most genes for biosynthesis of these biothiols and for general sulfur metabolism were down-regulated or no different from the unexposed cells, with the exception of up-regulation of cysE, which is the first step in the biosynthesis pathway from serine.

Fig. 8.

Amino acid biosynthesis. (see larger Additional file 1: Figure S22 and Additional file 11: Table S13 for details)

Methionine biosynthesis gene expression increased for 7 genes with HgCl_2, but 11 genes were down-regulated with PMA, especially metE dropping 187-fold with PMA at 30 min (Fig. 8 and Additional file 1: Figure S22). Expression of genes for histidine synthesis also responded differently to each mercurial, rising dramatically with HgCl₂ at 30 to 60 min. In contrast, all his genes expression dropped with PMA from 10 to 30 min. Genes for the synthesis of leucine, isoleucine, and valine had the opposite response, with most down-regulated with HgCl₂ but up-regulated with PMA. Expression of other amino acid biosynthetic pathways was largely unchanged or declined with both mercurials. Branched-chain (livKHMGF), dipeptide (dppABCDF), and oligopeptide (oppABCDF) transporters were also down-regulated for both mercurials, with greater relative negative fold-changes for PMA (Additional file 3: Table S5).

Inorganic ion transport and metallochaperones

Inorganic Hg(II) can displace beneficial thiophilic metals from their native binding sites in proteins, potentially affecting transport and disrupting transition metal homeostasis [23], leading to expression changes for non-ferrous metal cation and oxoanion transporters (Fig. 9 and Additional file 1: Figure S23 and Additional file 11: Table S13), iron homeostasis (Fig. 10 and Additional file 1: Figure S24 and Additional file 11: Table S13) and metal-binding proteins and enzymes (Additional file 13: Table S15).

Fig. 9.

Non-ferrous metals homeostases. (see larger Additional file 1: Figure S23 and Additional file 11: Table S13 for details)

Fig. 10.

Iron homeostasis. (see larger Additional file 1: Figure S24 and Additional file 11: Table S13 for details)

Inorganic mercury exposure releases labile iron, which could itself increase oxidative stress via Fenton chemistry under aerobic growth [23, 61]. Most iron uptake pathways declined early for both mercurials, consistent with the observed increase in expression of the Fur repressor. The cytochrome c maturation genes that transport heme to the periplasm (ccmABCDE) were also down-regulated for both mercurials. The putative ferrous iron and zinc efflux pump, fieF [62] increased 2-fold for HgCl₂ at 10 min only, suggesting it may have a transient role in restoring one or both of these homeostases.

There are two iron-sulfur (Fe-S) cluster assembly pathways in E. coli [63, 64]. Expression of the primary Isc system (iscRSUA, hscBA, and fdx) increased strongly for both mercurials, but with greater relative changes for HgCl₂ (Fig. 10 and Additional file 1: Figure S24 and Additional file 11: Table S13). The secondary Fe-S cluster assembly system sufABCDSE, which activates under oxidative stress or iron limiting conditions also increased greatly, but only for HgCl₂. These transcriptional responses confirm and extend biochemical findings [23] that Fe-S clusters are more vulnerable to inorganic mercury than to organomercurials and the cell quickly tries to repair this damage.

Expression of the zinc transporter zupT increased modestly in the 3- to 5-fold range for both mercurials during the first 30 min (Fig. 9 and Additional file 1: Figure S23 and Additional file 11: Table S13). In contrast, expression of the P-type ATPase zinc efflux pump, zntA [65] increased in the 20- to 40-fold range for both mercurials at 10 and 30 min and the periplasmic Zn-binding protein ZraP was up-regulated throughout recovery. E. coli has two copper/silver efflux systems, Cue and Cus [66]. Surprisingly, the Cus system genes (cusRS, cusCFBA) primarily used under anaerobic conditions were among the most down-regulated genes under PMA exposure. The Cue system consists of the multi-copper oxidase, CueO, and a P-type ATPase, CopA, both regulated by the MerR homolog, CueR. Genes cueO and copA were up-regulated approximately 20-fold with HgCl₂ at both 10 and 30 min whereas they increased 5-fold with PMA only at 10 min. The nickel uptake system [67] (nikABCDER) was also strongly down-regulated under PMA exposure conditions through all times although expression of repressor NikR was unchanged, except for a 3-fold increase with HgCl₂ at 10 min. Expression of the nickel and cobalt efflux gene, rcnA, increased with HgCl₂ or PMA. Manganese (mntH), and magnesium (mgtA, corA) uptake genes increased with both mercurials.

Inorganic anions used by E. coli include phosphate, sulfate, and molybdate and the genome also encodes genes for defense against arsenate, which acts as a phosphate mimic (Fig. 9 and Additional file 1: Figure S23 and Additional file 11: Table S13). Expression of the ABC phosphate transport system (pstSCAB) genes increased greatly for both mercurials, with PMA-provoked changes up to 165-fold, relative to unexposed condition, for the phosphate binding protein, pstS. The two-component phosphate regulatory system, PhoBR, was up-regulated for both mercurials; phoB changed up to 22-fold with HgCl₂ and 105-fold with PMA relative to the unexposed condition. Sulfate and thiosulfate uptake by the ABC transporter (cysPUWA) decreased strongly with HgCl₂ at 30 min and PMA at 10 and 30 min. Expression of molybdate uptake (modABC) increased with PMA during the first 30 min but only at 10 min with HgCl₂. The arsenate resistance operon cannot effect Hg(II) resistance, but was highly induced by both mercurials, perhaps through interacting with the three-cysteine metal-binding site of the ArsR repressor [68].

Surface functions

Cell wall biogenesis, porins, lps, efflux systems, and electrolyte balance

The transcriptional response of peptidoglycan, membrane biosynthesis, and cell division genes was similar for both mercurials (Additional file 1: Figure S25 and Additional file 11: Table S13). Expression increased for roughly 20% of lipid biosynthesis genes, including those for cardiolipin, and expression decreased for 20-30% of other lipid-related genes. Transcription of genes for murein synthesis (murCDEFGIJ) in particular declined for both mercurials during the first 30 min.

E. coli encodes several antibiotic resistance efflux systems that are up-regulated by mercury exposure (Fig. 11 and Additional file 1: Figure S26 and Additional file 11: Table S13). The multiple antibiotic resistance locus (marRAB), which increases drug efflux and also limits passive uptake by decreasing porin expression [69], was strongly up-regulated by both mercurials with greater fold-changes observed for PMA, relative to the unexposed condition. Though expression of some porin genes (ompC, ompF, ompT, ompW) was repressed, three non-specific porins (ompG, ompL, ompN) were up-regulated only by PMA. Genes from several TolC-dependent antibiotic efflux systems were up-regulated by both mercurials as well, including acrEF, emrD, emrKY, and several mdt genes [70]. HgCl₂ exposure alone also up-regulated two-component sensor genes (phoQP at 10 min and basSR at 60 min) that regulate genes involved in modification of the cell surface and increase polymyxin resistance [71], but most of these genes were down-regulated or unchanged for PMA.

Fig. 11.

Antibiotic resistance and outer membrane porins. (see larger Additional file 1: Figure S26 and Additional file 11: Table S13 for details)

The response to osmotic stress and maintenance of electrolyte balance are important membrane functions requiring adaptation in dynamic natural environments. During HgCl₂ exposure the expression of the sodium antiporter, NhaA, increased 4-fold at 10 min and the calcium/potassium antiporter, ChaA, was up-regulated 3-fold at 10 and 30 min (Fig. 9 and Additional file 1: Figure S23 and Additional file 11: Table S13). In contrast, expression of genes for transport of the major electrolyte, potassium, changed only modestly in some subunits of the kdp, kef, and trk systems, without an obvious response pattern. However, transcription of genes for defense against osmotic stress was uniformly up-regulated; betaine genes (betABIT and proP), osmBCEFY, and mechanosensitive channel proteins (mscL and mscS) increased for both mercurials, as did a putative osmoprotectant ABC permease (yehYXW) [72] only with HgCl₂ at 30 and 60 min (Additional file 3: Table S5).

Motility and biofilm

Nearly all flagellar component genes were strongly down-regulated for both mercurials, with greater negative fold-changes observed with PMA relative to the unexposed condition (Fig. 12 and Additional file 1: Figure S27). Only PMA increased expression of fimbriae and curli fiber genes, which alter motility and increase adhesion (Fig. 13 and Additional file 1: Figure S28) [73]. Fifteen genes up-regulated by PMA exposure were annotated as homologs of FimA, but with unknown function. FimA is the major structural component of fimbriae, but these genes may serve other functions. Motility genes whose expression dropped remained low until 60 min with HgCl₂, indicating that the structurally and energetically intensive motility systems are very slow to recover.

Fig. 12.

Flagella components and chemotaxis. (see larger Additional file 1: Figure S27 and Additional file 11: Table S13 for details)

Fig. 13.

Biofilm formation and fimbriae. (see larger Additional file 1: Figure S28 and Additional file 11: Table S13 for details)

HgCl₂ and PMA also provoked expression of several biofilm-related genes (Fig. 13 and Additional file 1: Figure S28 and Additional file 11: Table S13). The bhsA and bdcA loci were among the most highly up-regulated genes during HgCl₂ exposure, with a relatively greater fold-change than observed for PMA (Tables 2 and 3). Neither gene is well characterized, but independently each has been found to decrease biofilm formation and increase resistance to external stressors [74, 75]. Only PMA increased expression of genes for poly-β-1,6-N-acetyl-glucosamine (PGA) polysaccharide production [76] and biofilm related genes, ycgZ, ymgA, ariA, ymgC [77]. Thus, PMA elicits a broader response that potentially alters the cell surface and may increase adhesion and biofilm formation; in contrast HgCl₂ only inhibits motility and does not activate adhesion pathways. It is possible that some changes observed for motility and biofilm related genes following PMA-exposure are an artifact of the DMSO, but other studies suggest that solvent would have no effect or that much higher concentrations than used here would be required to induce these changes [56, 78].

Stress responses

Oxidative stress response and repair

There are two oxidative stress response pathways in E. coli, the oxyRS and soxRS regulons [61, 79]. OxyR, a LysR-family transcriptional regulator, uses a cysteine-pair to sense oxidative damage and regulates 49 genes when oxidized [80]. HgCl₂ exposure increased expression of 22 OxyR regulon genes at 10 min; these then declined to 13 genes by 60 min (Additional file 14: Table S16). In contrast, PMA provoked expression of 16 OxyR regulon genes at 10 and 30 min, but none at 60 min. OxyS, a small non-coding RNA regulated by OxyR, represses rpoS, fhlACD and other genes to prevent redundant induction of stress response genes [81]. The oxyS gene was among the most highly differentially expressed genes, increasing over 1000-fold with HgCl₂ at 10 and 30 min relative to the unexposed condition. Differential expression of oxyS was more modest with PMA having a relative increase of 10-fold at 10 min and 6-fold at 30 min.

The SoxRS regulon is the other oxidative stress response system in E. coli. SoxR, a MerR-family repressor-activator, uses the oxidation state of 2Fe-2S clusters to respond to superoxide (O₂⁻) stress and induce transcription of SoxS [82–85], which then transcriptionally regulates 53 genes [79, 86] (Additional file 14: Table S16). HgCl₂ or PMA exposure up-regulated 22 or 25 genes, respectively, at 10 min and these had declined to 13 or 0 genes, respectively by 60 min.

Key genes in these oxidative stress regulons differentially expressed upon mercury exposure include the ROS scavengers: catalase (katG), alkyl hydroperoxide reductase (ahpCF), and superoxide dismutase (sodA) (Fig. 14 and Additional file 1: Figure S29 and Additional file 11: Table S13). Thiol homeostasis genes included gor, grxA, and trxC (Fig. 14 and Additional file 1: Figure S29 and Additional file 11: Table S13). Iron homeostasis and the Fe-S cluster assembly and repair genes (fur, dps, fldA, fpr, hemH, sufABCDES, and yggX) were also up-regulated. PMA provoked comparatively lower fold-changes than HgCl₂ for grxA, trxC, ahpC, dps, fldA, hemH, and yggx. The manganese uptake protein, mntH, plays an important role in ROS resistance [87] and was up-regulated for both mercurials. Oxidation-resistant dehydratase isozymes, acnA and fumC [88, 89] also increased, but only for HgCl₂ exposure. Thus, both mercurials triggered the Oxy and Sox oxidative stress responses, but HgCl₂ elicited greater fold-changes overall than PMA compared to unexposed cells.

Fig. 14.

Oxidative stress defense and thiol homeostases. (see larger Additional file 1: Figure S29 and Additional file 11: Table S13)

Because mercury poisons the cellular thiol pool [23], we expected that regulation of redox homeostasis proteins such as glutaredoxins, thioredoxins and glutathione-related genes would respond to mercury exposure (Fig. 14 and Additional file 1: Figure S29). Glutaredoxin 1 (grxA) expression was up-regulated for both mercurials, with a greater fold-change observed for HgCl₂ relative to unexposed condition. In contrast, glutaredoxin 2 (grxB) was down-regulated for both mercurials, while glutaredoxin 3 (grxC) and glutaredoxin 4 (grxD) were up-regulated only for PMA. Thioredoxin reductase (trxB) was up-regulated 2-fold with PMA only at 30 min, but was up-regulated with HgCl₂ 8-fold (10 min) and 4-fold (30 min). Thioredoxin 1 (trxA) expression increased 2-fold only with PMA (10 min); in contrast to thioredoxin 2 (trxC), which was up-regulated for both mercurials, but had greater fold-change relative to the unexposed condition with HgCl₂ than with PMA. However, the thiol peroxidase (tpx) was up-regulated modestly for PMA, but did not change for HgCl₂. Thus, while each mercurial stresses the cell to maintain redox homeostasis, HgCl₂ exposure elicited greater responses.

Glutathione (GSH) serves as the cell’s redox buffer and as a scavenger of mercurials (Fig. 14 and Additional file 1: Figure S29 and Additional file 11: Table S13). Surprisingly, expression of GSH biosynthesis and utilization genes increased only modestly. The γ-glutamyltranspeptidase (ggt) increased late (60 min) by 4-fold only with HgCl₂. GSH synthase (gshA) did not change and gshB was up-regulated 2- or 3-fold for both mercurials only at 10 min. The GSH importer (gsiABCD) may be a salvage pathway to recover GSH and cysteine leaked into the periplasm by CydCD [90, 91], but it was down-regulated by HgCl₂ or PMA through 30 min. The GSH reductase (gor) increased only with HgCl₂ at 10 min and several GSH S-transferase genes involved in detoxification [92] (gstA, gstB, yfcF, yqjG, yibF, yncG) increased with both mercurials. Since all of these proteins have Hg(II)-vulnerable cysteines in their active sites, it is surprising that neither Hg(II) nor PMA-challenged cells provoked increased expression and suggests that their normal mRNA levels are sufficient to replenish them.

Genes with delayed up-regulation

Genes unchanged at 10 min but differentially expressed at both 30 and 60 min or 60 min alone may be those needed as cells transition out of stasis and towards normal growth (Additional file 15: Table S17). For HgCl₂ exposure, 95 genes were up-regulated and 140 genes were down-regulated that display this delayed response pattern. Approximately half of the up-regulated genes are involved in energy production, transport and metabolism pathways based on COG annotations. Roughly 45% of these delayed HgCl₂ provoked, up-regulated genes are the same as genes that were differentially expressed during the first 30 min of PMA exposure. This overlap is consistent with slower recovery of growth in HgCl₂ exposed cells and that some of the same pathways are used for recovery by both compounds. In contrast, for the more quickly recovering PMA exposure, of the genes that showed no change at 10 min only six were up-regulated at 60 min (Additional file 15: Table S17). Only two of these delayed-response genes for PMA exposure overlapped with up-regulated genes for HgCl₂ exposure.

Discussion

Mercury is a ubiquitous toxicant that serves no biologically beneficial role. Exposure to any form of mercury negatively impacts the health of organisms from microbes to humans. The biological effects of different forms of mercury are often conflated and methylmercury is assumed to be the most toxic form. However, the systemic biochemical and molecular differences between inorganic and organic mercury compounds have yet to be well characterized from exposure through recovery in a single model system.

Bulk differential effects on growth and gene expression

The sub-acute mercury exposure conditions used in this study were chosen by identifying a mercury concentration high enough to stop cells from doubling, but low enough to allow restoration of the pre-exposure growth rate within one-hour (~1 generation period) after exposure (Fig. 1a). Concentrations below 3 μM of either compound did not consistently inhibit growth and higher concentrations of HgCl₂ did not allow recovery within the desired time frame. The 3 μM Hg used in this study is well within the range that bacteria can experience chronically from dental amalgam fillings [93] and in highly contaminated environments, such as artisanal gold mining operations [8]. Mercury in tuna is 0.386 ppm compared to the proxy organomercurial, PMA, used here at 3 μM or 0.6 ppm [94].

PMA-exposed cells recovered exponential growth faster (Fig. 1) than those with equimolar exposure to HgCl₂, perhaps owing to lower uptake of PMA (Additional file 1: Table S2). However, PMA-exposed cells differentially expressed more genes than HgCl₂ exposed cells during the first 30 min of exposure (Fig. 1b). These results agree with observations in C. elegans, where MeHg exposure resulted in four times more DEGs than did HgCl₂ for all concentrations tested [95]. However, in contrast to E. coli, whose growth was inhibited more by inorganic HgCl₂, in C. elegans the effective toxic concentration of methylmercuric chloride was lower than for HgCl₂ [95]. The large number of significant DEGs in response to mercury exposure is greater than the response to hydrogen-peroxide [96] or nitric-oxide [97], but other types of chemical exposures to organic acids [98] and volatile organic compounds [99] in E. coli have resulted in similar numbers of DEGs to mercury exposure and the stress response sigma factor RpoS has been shown to regulate up to 23% of the genome alone [100].

We found that most DEGs peaked at 10 min after exposure for both compounds with HgCl₂ provoking more down-regulated genes and PMA yielding more up-regulated genes throughout the exposure period (Fig. 1b). Even though the optical density (OD) of the HgCl₂ exposed culture showed no growth recovery from 10 min to 30 min, DEGs decreased by 22%, while PMA-exposed cells over the same period had a moderate increase in OD, but only an 8% decrease in DEGs (Fig. 1). In contrast in a eukaryotic system, the livers of HgCl₂ exposed zebrafish continuously increased in DEGs throughout the observed 96 h exposure period as mercury accumulated in their cells [101].

In E. coli, during the first 30 min post-exposure, 50-70% of both up- and down-regulated genes were the same for both compounds (Fig. 2), but at the level of individual genes there were both qualitative and quantitative differences in expression (Additional file 3: Table S5), consistent with idiosyncratic transcriptional responses to each compound. The nematode C. elegans also manifested distinct and even some opposite transcriptional responses to inorganic and organic mercury exposure in a single end-point microarray experiment [24].

As there are not yet other studies of the global transcriptional response of a bacterium to mercury exposure, on the basis of the findings in eukaryotes and our proteomic work [23] we have organized our observations here into those we had expected and those we did not expect from any yet published work.

Expected and unexpected gene-specific changes

Expected transcriptional changes:

Thiol homeostasis.

The millimolar cytosolic pool of glutathione (GSH) can sequester mercurials and thereby protect protein thiols from binding strongly to these soft metal toxicants. However, if the GSH pool becomes depleted by mercury complexation, the cell loses this primary defense mechanism. Since proteins of the stress response and repair pathways all contain active site thiols, often as part of Hg(II)-vulnerable Fe-S centers, it is not obvious how a cell that has lost much of its available thiols to Hg(II) chelation can restore its metabolism. Given this, we expected cysteine and glutathione biosynthesis pathways to be up-regulated. However, cysteine biosynthesis was down-regulated (Fig. 8 and Additional file 1: Figure S22 and Additional file 11: Table S13) and GSH biosynthesis was mostly unchanged (Fig. 14 and Additional file 1: Figure S29 and Additional file 11: Table S13) for both compounds, in contrast to the eukaryotic response to mercury [101–103] and H₂O₂ exposure [96], which increase GSH and metallothionein production. However, although thiol biosynthesis did not increase, genes involved in maintaining cellular thiol homeostasis did increase (Fig. 14 and Additional file 1: Figure S29 and Additional file 11: Table S13); thioredoxin (trxC) and glutaredoxin (grxA) were among the most highly up-regulated genes with HgCl₂ and PMA exposure. Others have also found in E. coli that glutathione reductase increased with HgCl₂ and both compounds increased expression of glutathione oxidoreductase and S-transferase genes, which protect against oxidative stress and xenobiotics [104].

Iron homeostasis.

We also expected inorganic mercury to disrupt iron-sulfur clusters with consequent effects on Fe homeostasis generally [23, 105]. Iron uptake was down-regulated with both mercurials, consistent with excess intracellular free Fe(II) and general oxidative stress, but expression of the uptake repressor (fur) was only up-regulated for HgCl₂ (Fig. 10 and Additional file 1: Figure S24). Fur expression is activated by either OxyR or SoxS [96, 106] and Fur represses Fe uptake pathways with ferrous iron as a co-repressor [107]. Fur can also bind other divalent metals [108], so Hg(II)-Fur might mimic Fe-Fur as an iron uptake repressor under these conditions to limit Fenton-mediated damage from excess iron. Although both mercurials increased expression of the primary Fe-S cluster assembly and repair system (isc), only HgCl₂ induced the secondary system (suf), which is normally induced under oxidative stress or iron limiting conditions [63, 109] (Fig. 10 and Additional file 1: Figure S24 and Additional file 11: Table S13). Also, only HgCl₂ exposure increased expression of iron storage proteins: ferritin, bacterioferritin, and Dps (Fig. 10 and Additional file 1: Figure S24). The DNA binding protein Dps which binds free iron to protect DNA from ROS damage [110] was one of the most highly up-regulated genes with HgCl₂ exposure (Table 1).

Oxidative stress response.

The known close link between iron homeostasis and oxidative stress [61] explains the large fold-changes observed upon HgCl₂ exposure in genes that respond to oxidative stress (Additional file 14: Table S16) and echoes mercury’s long known stimulation of oxidative damage in rat kidney mitochondria [111]. The small non-coding RNA oxyS was the second most highly up-regulated gene upon HgCl₂ exposure with differential expression more than 100-fold greater than observed for PMA (Table 1). The ROS scavenger ahpF was also highly up-regulated, along with katG (early) and sodA (delayed) but only for HgCl₂ (Fig. 14 and Additional file 1: Figure S29 and Additional file 14: Table S16). Other ROS resistant enzymes, aconitase A [89] and fumarase C [112] (Additional file 14: Table S16) also increased only for HgCl₂, as did the manganese-dependent alternative ribonucleotide reductase genes (nrdHIEF) [113]. The glutaredoxin-like protein that functions like thioredoxin, nrdH [114], was highly up-regulated by HgCl₂ and might support other thioredoxin and glutaredoxin proteins. These striking differences in gene expression illuminate how E. coli modulates expression of specific genes not only to deal with compromised function of specific HgCl₂ modified proteins, but also to manage the consequent cascade of reactive oxygen species.

Heat shock response.

Mercurials bound to protein cysteines could disrupt protein folding, subunit assembly, and allosteric movements [52, 115] and inorganic mercury can crosslink neighboring cysteines leading to aggregation [51]. Increased expression of heat shock response genes was expected as a consequence of such anticipated protein misfolding problems [116]. Indeed, expression of heat shock chaperonins and protease genes increased for both mercurials, with more genes up-regulated early in response to HgCl₂ than to PMA (Fig. 6 and Additional file 1: Figure S12 and Additional file 11: Table S13). Genes for the small chaperone-like proteins, ibpA and ibpB, were among the most highly increased for both compounds, especially for HgCl₂ (Table 1), consistent with their role in aiding Lon protease in the degradation of misfolded proteins [117–119].

Translational apparatus.

Thiophilic Cd²⁺ exposure in E. coli has been shown to decrease expression of ribosomal proteins [120]. In our proteomics work (Zink et al. in preparation) we observed 14 r-proteins (7 for each ribosomal subunit) that formed stable adducts with either PMA or Hg(II), so it was reasonable to expect this to be reflected in transcription of r-proteins. Indeed, HgCl₂ exposure repressed expression of up to 83% of r-protein genes at 10 min and 74% at 30 min (Fig. 5, Additional file 1: Figure S11, and Additional file 12: Table S14), whereas PMA only transiently repressed expression of 41% of r-proteins at 30 min. Divalent inorganic mercury’s ability to cross-link proteins may interfere with ribosome assembly resulting in translational feedback and repression of r-proteins transcription. Disruption of ribosome assembly could also contribute to the slower recovery of growth after inorganic Hg(II) exposure.

Energy production.

The dependence of most energy production pathways on redox-active transition metals and redox-active sulfur compounds made them obvious targets of mercurial disruption, e.g. three ATP-synthase subunits form stable adducts after in vivo exposure to Hg(II) or PMA (Zink et al. in preparation). Expression of genes within this functional category was largely down-regulated early in exposure, with all nine ATPase subunits down-regulated for HgCl₂ (10 min) and eight down-regulated for PMA (30 min) (Fig. 7 and Additional file 1: Figure S13). Although others have found that Cd exposure in E. coli repressed aerobic energy metabolism genes and induced anaerobic pathways [120], we found that both aerobic and anaerobic energy metabolism were repressed by HgCl₂ and PMA. Even though expression of the oxygen-sensing fnr [121] and aer [122, 123] activators of the anaerobic shift were moderately up-regulated for PMA and unchanged for HgCl₂ (Additional file 3: Table S5). Similarly, glucose metabolism genes were also predominantly down-regulated during early periods for both compounds, especially with PMA exposure (Additional file 1: Figure S14). Thus, with severely compromised energy production systems, it is not surprising that amino acid, carbohydrate and nucleotide metabolism genes, and the energy-dependent transport of these molecules (Fig. 3 and Additional file 4: Table S6), are also largely depressed initially.

Homeostases of non-ferrous metals.

We expected mercurials to disrupt electrolyte balance [23], but expression of the potassium efflux pumps’ subunit genes (kcpABC, kefBC, and trkAGH) were not uniformly up-regulated, although the need to restore the pH balance was indicated by transiently increased expression of the H⁺/Na⁺ antiporter (nhaA) for both compounds (Fig. 9, Additional file 1: Figure S23 and Additional file 3: Table S5). It may be that normal levels of the proteins involved in maintaining cellular electrolyte balance are sufficient to respond to mercury exposure and a significant change in transcriptional expression is not required for these genes.

Mercury is also expected to disrupt non-ferrous metal homeostasis because it can displace other metals, such as zinc and copper, as enzyme cofactors [124, 125]. Expression of metal uptake genes decreased and of metal efflux genes increased for zinc, copper, nickel and cobalt, with relatively greater fold-changes occurring with HgCl_2. Zinc efflux by ZntA is regulated by the MerR homolog ZntR, which can respond to Hg(II) [126], but has not been shown to confer resistance to Hg(II) exposure. Up-regulated periplasmic transition metal binding proteins, ZraP [127] and ZinT [128], use histidine residues to coordinate metal binding and all cysteine residues present in either protein are involved in structural disulfide bonds that prohibit availability for binding metals. Thus, these periplasmic metal binding proteins lack requisite thiol ligands [23] to compete for Hg effectively with periplasmic glutathione [90, 129, 130]. Their increased transcription here likely reflects their control by a complex suite of redox and other stress regulators [86] provoked by Hg exposure as reported above. Manganese may protect iron metalloenzymes under oxidative stress conditions [87] and Mn uptake by mntH, as part of the OxyR regulon, was correspondingly up-regulated for both compounds in response to mercury-induced oxidative stress.

Unexpected transcriptional changes:

Motility and chemotaxis.

Energetically costly flagellar motility and chemotaxis were strongly down-regulated by both mercurials and were among the slowest to recover normal transcription levels (Fig. 12 and Additional file 1: Figure S27 and Additional file 11: Table S13). Motility gene expression is regulated by σ²⁸ (fliA) and FlhDC [131] and the expression of these two regulatory genes declined with HgCl₂ but was unchanged with PMA. Repression of motility may occur through sigma factor competition for binding to RNAP between σ²⁸ and increased expression of σ^S [132] and/or through repression of the flagellar transcriptional activator FlhDC by increased expression of the small ncRNAs oxyS and gadY [133]. Interestingly, HgCl₂ exposure impaired locomotion in C. elegans [24], although through a very different mechanism of motility from E. coli.

Surface appendages and biofilm synthesis.

Surprisingly, there were large increases in expression of genes involved in biofilm formation and adhesion or dispersal (Fig. 13 and Additional file 1: Figure S28 and Additional file 11: Table S13). Expression of bhsA and bdcA, which function in biofilm dispersal or reduced biofilm formation [74, 75], were the first and third, respectively, most up-regulated genes by HgCl₂ (Table 1) and were also up-regulated for PMA, but with relatively smaller fold-changes (Table 2). Expression of bhsA is also up-regulated by other diverse stressors and may decrease cell permeability [75, 134]. PMA exposure especially increased expression of genes for the polysaccharide PGA, which aids in adhesion in biofilm formation [76], and other biofilm formation (ycgZ, ymgA, ariA, ymgC) genes [77] (Fig. 13 and Additional file 1: Figure S28 and Additional file 11: Table S13).

Expression of fimbriae (fim) and curli fibers (csg), important for adhesion in biofilm formation [73] were also up-regulated only by PMA (Fig. 13 and Additional file 1: Figure S28), as were 15 of 22 FimA homologs of unknown function. Outer membrane vesicle formation (OMVs) could also play a role in detoxification, since an increase in formation of these vesicles has been associated with heat shock, oxidative stress response, and biofilm formation [135], which are responses up-regulated to varying degrees by both mercurials. These are distinct differences between PMA and HgCl₂ response. PMA provocation of biofilm formation and adhesion genes might be an artifact of its DMSO solvent, but it is not obvious why HgCl₂ induces such high increases in biofilm dispersal genes.

Phosphate metabolism.

Phosphate uptake genes were among the most highly up-regulated genes for PMA exposure (Fig. 9, Additional file 1: Figure S23, and Table 2). The PhoBR two-component system controls expression of phosphate transport genes, as well as some genes that increase virulence including those for fimbriae and biofilm formation [136]. Since expression of PhoBR and its regulon increases under phosphate limiting conditions [137], it may be that PMA inhibits phosphate uptake by an unknown mechanism, possibly through direct interaction with highly up-regulated PstS or this could be an artifact of DMSO.

Amino acid biosynthesis.

Expression of most amino acid pathways was down-regulated by both compounds, but a few responded uniquely to each mercurial (Fig. 8 and Additional file 1: Figure S22 and Additional file 11: Table S13). Since methionine auxotrophy occurs under oxidative stress due to ROS susceptibility of methionine synthase (MetE) [138], expression of methionine biosynthesis genes may have increased with HgCl₂ due to a stronger oxidative stress response than PMA. However, since PMA did up-regulate some oxidative stress-related genes, it is curious that Met operon expression was down-regulated under PMA exposure. Next to its affinity for cysteine sulfur, Hg(II) binds the imino nitrogen of histidine very strongly [139], so it was intriguing that histidine biosynthesis genes were also up-regulated by HgCl₂ but down-regulated by PMA. It remains unclear how these differences or the opposite responses for leucine, isoleucine and valine biosynthesis help the cell survive mercurial exposure.

Miscellaneous genes.

Multiple antibiotic efflux systems and polymyxin resistance surface modifications were up-regulated by HgCl₂ exposure, and even more so by PMA (Fig. 11 and Additional file 1: Figure S26 and Additional file 11: Table S13). Chronic mercury exposure contributes to the spread of multiple antibiotic resistant bacteria through co-selection of plasmid-borne antibiotic and mercury resistance genes [140, 141]. Increased expression of antibiotic resistance and surface components hint that low-level mercury exposure could prime cells for increased antibiotic resistance. However, the ubiquity of plasmid- and transposon-borne Hg resistance loci suggests that expression of these chromosomal genes offers insufficient protection against the antibiotic or mercurial levels encountered in clinical practice.

A handful of vestigial e14 or CPS-53 prophage genes were up-regulated by HgCl₂ (Table 1) or PMA (Additional file 3: Table S5), respectively. Some are known to increase resistance to osmotic, oxidative, and acid stressors [142, 143], but their roles and mechanisms have not been well defined.

Differential expression of genes required for the same functional protein complex.

In many instances we observed that transcripts for subunits of the same enzyme, protein complex, or component of a tightly articulated pathway were differentially expressed. In some cases these proteins lie in distinct transcripts, which may experience different turnover rates and in other cases the differences could be due to transcriptional polarity. We have chosen not to deal explicitly with such paradoxes in this work, which is sufficiently complex as it is, but will address them in future work.

Conclusions

The effects of mercury exposure in multicellular organisms have long been studied at the physiological level but a global, fine grained understanding of the differences in the precise biochemical sequelae of inorganic and organic mercury exposure has been lacking. This study is the first to examine not only the global transcriptional response differences between inorganic mercury (HgCl₂) and an organomercurial (phenylmercuric acetate) in a model microorganism, but also first to examine longitudinally how the cell recovers from these chemically distinct compounds. Taken together with global identification of vulnerable protein targets (Zink et al... in preparation) and of damage to thiol and metal ion homeostasis upon acute mercurial exposure [23], the current work provides a quantitative systems-level description of the effects of in vivo mercury exposure in E. coli. What was striking and most challenging with this study was the breadth and diversity of the systems whose expression was affected by these two chemically distinct mercurials. Sub-acute exposure influenced expression of ~45% of all genes with many distinct responses for each compound, reflecting differential biochemical damage by each mercurial and the corresponding resources available for repair. Energy production, intermediary metabolism and most uptake pathways were initially down-regulated by both mercurials, but nearly all stress response systems were up-regulated early by at least one compound. These results echo the wide functional variety of proteins stably modified by these mercurials owing to the widespread occurrence of cysteines found in nearly all E. coli proteins. Microbiome studies are rapidly unveiling the importance of commensal bacteria to the health of all higher organisms. Our findings in this model commensal organism provide insights into how chronic mercury exposure might affect such complex microbial communities and, consequently, the health of the host. This work also serves as a foundation for studies now underway of how the widely found mobile Hg resistance (mer) locus assists the cell in recovery from Hg exposure.

Abbreviations

COGs

Clusters of orthologous groups

CVAA

Cold vapor atomic absorption

Cys

Cysteine

DEGs

Differentially expressed genes

DMSO

Dimethyl sulfoxide

ETC

Electron transport chain

GOFs

Gene-ontology functions

GSH

Glutathione

Hg

Mercury

HgCl₂

Mercuric chloride

HSP

Heat shock protein

LB

Luria-Bertani medium

MDR

Multidrug resistance

ncRNA

Non-coding RNA

NGS

Next generation sequencing

NM3

Neidhardt MOPS minimal medium

PGA

Poly-β-1,6-N-acetyl-glucosamine

PhHg

Phenylmercury

PMA

Phenylmercuric acetate

RNAP

RNA polymerase

Authors’ contributions

SL conceived and designed experiments, prepared biological samples, extracted ribosomal depleted RNA for RNA-Seq, performed all data analysis, and drafted manuscript. AOS was a major contributor in experimental design, feedback on data analysis, and in editing the manuscript. Both authors read and approved the manuscript.

Ethics approval and consent to participate

Not applicable

Consent for publication

Not applicable

Competing interests

The authors declare that they have no competing interests.

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.