Extracellular DNA release, quorum sensing, and PrrF1/F2 small RNAs are key players in Pseudomonas aeruginosa tobramycin-enhanced biofilm formation

Abstract

Biofilms are structured microbial communities that are the leading cause of numerous chronic infections which are difficult to eradicate. Within the lungs of individuals with cystic fibrosis (CF), Pseudomonas aeruginosa causes persistent biofilm infection that is commonly treated with aminoglycoside antibiotics such as tobramycin. However, sublethal concentrations of this aminoglycoside were previously shown to increase biofilm formation by P. aeruginosa, but the underlying adaptive mechanisms still remain elusive. Herein, we combined confocal laser scanning microscope analyses, proteomics profiling, gene expression assays and phenotypic studies to unravel P. aeruginosa potential adaptive mechanisms in response to tobramycin exposure during biofilm growth. Under this condition, we show that the modified biofilm architecture is related at least in part to increased extracellular DNA (eDNA) release, most likely as a result of biofilm cell death. Furthermore, the activity of quorum sensing (QS) systems was increased, leading to higher production of QS signaling molecules. We also demonstrate upon tobramycin exposure an increase in expression of the PrrF small regulatory RNAs, as well as expression of iron uptake systems. Remarkably, biofilm biovolumes and eDNA relative abundances in pqs and prrF mutant strains decrease in the presence of tobramycin. Overall, our findings offer experimental evidences for a potential adaptive mechanism linking PrrF sRNAs, QS signaling, biofilm cell death, eDNA release, and tobramycin-enhanced biofilm formation in P. aeruginosa. These specific adaptive mechanisms should be considered to improve treatment strategies against P. aeruginosa biofilm establishment in CF patients’ lungs.

Introduction

Bacterial biofilm forms a highly structured community of cells that are attached to each other and/or a surface and are enclosed in a complex matrix of extracellular polymeric substances (EPS).1,2 Biofilms enable bacteria to colonize different environments and are prevalent in natural, industrial and medical environments. Importantly, biofilms have emerged as critical in chronic infections. The traits of bacteria within biofilms are distinct from those of their planktonic counterparts, which include an increased resistance to both biocide agents and antibiotics, the development of physical and social interactions, enhanced rate of gene exchange and selection for phenotypic variants.3,4 In many bacterial species, biofilm formation responds to a variety of environmental cues including nutritional availability, host-derived signals or, in some cases, to nonlethal concentrations of antibiotics.5,6,7,8 The process of biofilm development is coordinated by molecular pathways involving second-messenger signaling, cell-to-cell quorum sensing (QS) signaling, two-component systems and small noncoding RNAs (sRNAs).6 Interestingly, antibiotics at levels below the minimal inhibitory concentration (referred to hereafter as sub-MIC) have the ability to trigger the alteration of multiple physiological processes including biofilm formation, virulence, and gene expression, which can lead to bacterial genetic and phenotypic resistance.9,10,11,12 Sub-MICs of antibiotics with different chemical structures and modes of action induce biofilm formation in common clinical pathogens such as Staphylococcus aureus, Enterococcus faecalis, Escherichia coli, and Pseudomonas aeruginosa, among others.5,11

P. aeruginosa is a problematic Gram-negative pathogen representing a serious threat to individuals and public health. This opportunistic pathogen causes both acute and chronic infections that are strongly related to its planktonic and biofilm lifestyles, respectively. Within the lungs of cystic fibrosis (CF) individuals, biofilms are gradually formed by P. aeruginosa cells surrounded by a self-produced matrix of EPS such as polysaccharides, proteins, extracellular DNA (eDNA), metabolites, and siderophores.2,13,14,15 As a result of their ability to form biofilms and their high tolerance levels towards a broad spectrum of antimicrobials, P. aeruginosa chronic lung infections are almost impossible to eradicate.13,16,17 Tobramycin, an aminoglycoside antibiotic, is used in the treatment of P. aeruginosa infections.18 However, exposure to sub-MIC of this aminoglycoside19,20,21,22 and of other antibiotics such as quinolones23 and tetracycline20,21 enhances P. aeruginosa biofilm formation. Conversely, some other antibiotics such as polymyxin B, carbenicillin, and chloramphenicol, do not impact biofilm development.19

Based on microarray studies, tobramycin at the sub-MIC dose of 1 µg ml−1 led to altered expression of genes that are mainly involved in adaptation and protection processes in P. aeruginosa grown under planktonic conditions.21 Additionally, a recent study assessed the proteome response of planktonic cells of P. aeruginosa exposed to 0.1, 0.5, and 1 µg ml−1 sub-MIC of tobramycin.24 The authors identified higher abundances of multiple heat-shock proteins, proteases and proteins related to amino acid catabolic pathway. In contrast, they observed lower abundances of proteins associated with nucleotide metabolism, tricarboxylic acid (TCA), carbon metabolism and energy derivation, and electron transport activities. A small number of proteins were common to the proteomes produced at different sub-MICs of tobramycin while some proteins showed dose-dependent responses. It is worth to mention that aminoglycosides at sub-MICs can also induce other changes in P. aeruginosa physiology, including swimming and swarming motilities and the induction of the type VI secretion system (T6SS).20,21 Noteworthy, most of these studies have been conducted on bacteria grown under planktonic conditions. However, since bacteria are thought to adopt predominantly the biofilm lifestyle in nature and in infected host, it is crucial to perform studies on bacteria grown under sessile conditions.

In this context, we sought to elucidate adaptive mechanisms shaping the tobramycin-enhanced biofilm formation in P. aeruginosa. Remarkably, our observations support a potential adaptive mechanism in which the 4-hydroxy-2-alkylquinolines (HAQs) molecules and PrrF sRNAs are key players in eDNA release, presumably resulting from cell death which finally trigger changes in the biofilm architecture.

Results

Tobramycin exposure leads to changes in biofilm architecture, biovolume and thickness

Previous studies showed enhanced P. aeruginosa biofilm formation upon exposure to tobramycin and other aminoglycosides by using colorimetric assays based on crystal violet staining.19,20,21 To observe the biofilm architectures and to quantify the biovolumes as well as the thicknesses of the biofilms, confocal laser scanning microscopy (CLSM) and COMSTAT image analyses were performed. First, we determined that the MIC of tobramycin for the P. aeruginosa wild-type H103 strain is 2 μg ml−1. Then, we grew P. aeruginosa H103 biofilms in glass bottom microplates under static conditions for 24 h in the presence of 0−2 μg ml−1 of tobramycin. Under our conditions, sub-MICs of tobramycin (0.5−1 μg ml−1) increased the presence of three-dimension (3D) structures in the biofilms (Fig. 1a). Consistently, at 0.7, 0.8, and 0.9 μg ml−1 tobramycin, the biofilm biovolumes, the maximum thicknesses, and the average thicknesses reached utmost significant increases compared to that of tobramycin-free biofilms (Fig. 1b). Thus, the concentration of 0.8 μg ml−1 of tobramycin was selected as the sub-MIC for all subsequent experiments.

Fig. 1
figure1

Effect of sub-MICs of tobramycin on biofilm formation by P. aeruginosa. a CLSM images of 24-h-old biofilms as a function of different concentrations of tobramycin. For each concentration, a 3D view along the x, y and z axes is displayed. Images show representative data from at least three independent biofilm assays. Scale bars = 20 µm. b COMSTAT image analyses were performed to determine maximum thicknesses (μm), average thicknesses (μm), and total biovolumes (μm3 μm−2). The error bars represent the standard error of the means (SEMs) and are the result of the analysis of three views of each of the three independent biological assays. Statistics were achieved by a two-tailed t test: , P = 0.0001 to 0.001; , P = 0.001 to 0.01; , P = 0.01 to 0.05; NS (not significant), P ≥ 0.05

Extracellular DNA release and cell biofilm death increase in presence of tobramycin

We then asked whether eDNA, a major structural component of the P. aeruginosa biofilm matrix,14,15,25 contributes to the observed enhanced biofilm formation in response to tobramycin. CLSM and COMSTAT image analyses were used to evaluate the in situ eDNA level. The bacterial cells were labeled with the green fluorescent nucleic acid stain SYTO 9, and DDAO, a red fluorescent probe unable to cross the cell membranes, was used for eDNA staining. Figure 2a shows that the red labeling is more intense in a biofilm grown for 24 h in the presence of tobramycin than in a tobramycin-free biofilm, revealing a higher eDNA content in the first condition. Moreover, the red fluorescence was visible at the periphery of 3D structures in the presence of tobramycin, showing that eDNA might be involved, at least partly, in modifying the biofilm architecture in response to tobramycin. In the absence of tobramycin, a yellow coloration due to the superposition of the green (bacteria) and red (eDNA) fluorescence was observed, suggesting that eDNA was mostly localized within the biofilm. COMSTAT analyses indicated a 2.1-fold relative increase in eDNA abundance when biofilms were exposed to sub-MIC of tobramycin (Fig. 2b). To assess the impact of eDNA on biofilm formation, biofilms were grown with tobramycin, DNase I (100 μg ml−1), or tobramycin and DNase I simultaneously, and were compared to untreated biofilms. The addition of DNase I at the onset of biofilm formation decreased the biovolume of 24-h-old tobramycin-free biofilms by 27% (Fig. 2c). Interestingly, when biofilms were formed simultaneously in presence of DNase I and tobramycin, the total biofilm biovolume was reduced by 42.4% compared to biofilm formed under tobramycin exposure without DNase I (Fig. 2c). Similarly, COMSTAT images analyses indicated that while the eDNA relative abundance in biofilms of H103 grown in the presence of DNase I was decreased by about 20.2%, it was reduced by 33.5% in biofilms grown with both DNase I and tobramycin compared to tobramycin-exposed biofilms without DNase I. These results indicate that eDNA release contributes to a certain extent to tobramycin-enhanced biofilm formation by P. aeruginosa H103. Moreover, we attempted to assess if the eDNA release occurs through cell lysis. To this end, cell death was evaluated using the Live/Dead staining kit (Fig. 2d). COMSTAT analyses of CLSM images revealed that cell death was significantly increased from 1 to 1.25-fold (by about 25%) in P. aeruginosa H103 biofilms grown in the presence of tobramycin compared to tobramycin-free biofilms (Fig. 2e). Altogether, these data indicate that tobramycin at sub-MIC induced eDNA release, most likely through cell lysis, thereby modifying the matrix composition, which might contribute at least in part to the increased biofilm formation.

Fig. 2
figure2

Sub-MIC of tobramycin leads to increased eDNA release and cell death in P. aeruginosa biofilm. a Representative CLSM 3D-top and side views of eDNA accumulation in 24-h-old P. aeruginosa biofilms exposed to tobramycin (0.8 μg ml−1) alone, DNase I (100 μg ml−1) alone or tobramycin and DNase I simultaneously, compared to untreated biofilms. Prior to image acquisition by CLSM, P. aeruginosa biofilm cells were labeled in green with SYTO 9 and the eDNA was stained in red with DDAO. Scale bars = 20 µm. CLSM images were analyzed using the COMSTAT software to quantify b the eDNA relative abundances relatively to biofilm biovolume values. Error bars represent standard error of the means (n = 3) and c the biofilm biovolumes. Error bars represent standard error of the means (n = 3). d CLSM micrographs of P. aeruginosa biofilms grown in the absence of tobramycin (left panel) and in the presence of drug (right panel) stained using the LIVE/DEAD® BacLightTM Bacterial Viability Kit. Green fluorescent cells are viable, whereas red fluorescent cells have compromised cell membranes. Scale bars = 20 µm. e The cell death in biofilms was determined by COMSTAT images analyses. Values of nonviable biovolumes were normalized to total biovolumes. Error bars represent standard error of the means (n = 3). Statistics were achieved by a two-tailed t test: , P = 0.001 to 0.01; , P = 0.01 to 0.05

Proteomic profiling of tobramycin-enhanced biofilm formation suggests a complex adaptive physiology

To gain further insights into the tobramycin-enhanced biofilm formation potential adaptive mechanisms, the whole biofilm proteome was analyzed. The obtained results allowed the identification of 174 proteins with at least a twofold change in abundance in presence of sub-MIC tobramycin. Among these, 118 proteins showed increased abundances (Supplementary Table 1) while 56 were less abundant (Supplementary Table 2). An enrichment analysis with respect to PseudoCAP functional classes26 was performed for the reduced and increased-abundance proteins, respectively (Supplementary Fig. 1). The majority of enriched PseudoCAP functions for increased-abundance proteins belong to the categories of “secreted factors”, “adaptation and protection”, “antibiotic resistance and susceptibility”, “chaperones & heat shock proteins”, “amino acid biosynthesis and metabolism”, and “biosynthesis of cofactors, prosthetic groups and carriers” (Supplementary Fig. 1). By contrast, for reduced-abundance proteins, the PseudoCAP functional classes belong to “transcription, RNA processing, and degradation”, “energy metabolism”, “amino acid biosynthesis and metabolism”, and “carbon compound catabolism” (Supplementary Fig. 1). Next, a protein−protein interaction network was determined for proteins that were differentially produced in tobramycin-exposed biofilm. One hundred and ninety-one functional connections were inferred between 111 of the 174 proteins by selecting connections over a threshold of 0.7 of confidence combined score. The resulting string network was visualized within Cytoscape (version 3.2.1)27 (Fig. 3). The obtained results suggest a high number of interactions between the identified proteins which might be involved in the tobramycin-induced biofilm formation in P. aeruginosa. Interestingly, the proteome response to sub-MIC tobramycin treatment revealed increased levels of proteins associated with QS signaling networks, phenazine biosynthetic pathways and extracellular proteases (Supplementary Table 1; Fig. 3). On the other hand, the proteome analysis showed a decreased abundance of some proteins that are involved in central metabolism, including proteins associated with glycolysis, TCA cycle, and anaerobic metabolism (Supplementary Table 2; Fig. 3). Noticeably, the proteome of tobramycin-exposed P. aeruginosa biofilm showed reduced accumulation of ribonucleases RNase E (PA2976), RNase R (PA4937), and PNPase (PA4740) (Supplementary Table 2; Fig. 3), suggesting a possible reduced catabolism of RNAs. Overall, these proteomic data revealing alterations in the abundance of numerous proteins suggest complex adaptive mechanisms underlying tobramycin-increased biofilm development by P. aeruginosa.

Fig. 3
figure3

Protein−protein interaction network for highly differentially accumulated proteins in the P. aeruginosa biofilm cultures exposed to sub-MIC level of tobramycin. Nodes are colored according to the protein abundance (fold change). Nodes highlighted in green color correspond to the overaccumulated proteins whereas the nodes in red color represent the underaccumulated proteins. Edges indicate protein−protein interactions

Tobramycin-enhanced biofilm formation is associated to production of QS molecules

Since QS signaling molecules have been reported to be involved in eDNA release via subpopulation cell lysis,28 the ability of tobramycin to increase the production of QS-related molecules in colony biofilms of H103 strain was determined using LC-MS/MS quantification. As shown in Fig. 4a, tobramycin significantly increased the production of the two main P. aeruginosa N-acyl-homoserine lactones (AHLs), N-(3-oxododecanoyl)-l-homoserine lactone (3-oxo-C12-HSL), and N-butanoyl-l-homoserine lactone (C4-HSL). Furthermore, the major molecules from the HAQs family, namely 3,4-dihydroxy-2-heptylquinoline (termed the Pseudomonas quinolone signal (PQS)), its precursor 4-hydroxy-2-heptylquinoline (HHQ) and 4-hydroxy-2-heptylquinoline N-oxide (HQNO) were all significantly more abundant upon tobramycin exposure (Fig. 4b). Accordingly, the proteomic analyses revealed an enhanced production of PqsB (PA0997), PqsC (PA0998), and PqsD (PA0999) that are involved in HHQ biosynthesis (Supplementary Table 1; Fig. 3). This was also the case for both PqsH (PA2587), responsible for the conversion of HHQ into PQS,29,30 and PqsL (PA4190), which is required for HQNO biosynthesis31 (Supplementary Table 1; Fig. 3). These results provide evidence that sub-MIC of tobramycin induces the production of QS-related molecules, especially PQS and HQNO that might be involved in eDNA release and/or cell lysis, leading partly to the observed tobramycin-increased biofilm formation in P. aeruginosa. To support this hypothesis, a pqs mutant strain (ΔpqsA) was constructed to determine the impact of HAQ molecules on biofilm formation and eDNA release in tobramycin-exposed biofilms (Fig. 4c). As expected, HAQs levels determined by LC/MS-MS were shown to be abolished in ΔpqsA biofilm exposed or not to tobramycin compared to HAQs levels of H103 wild-type strain (Supplementary Table 3). The ΔpqsA mutant displayed reduced biofilm biovolume (by about 38%) compared to H103. The presence of tobramycin in ΔpqsA biofilm cultures increased the biovolume compared to ΔpqsA tobramycin-free biofilms as in the case of H103 treated or not with tobramycin but in a minor rise proportion (Fig. 4d). Noticeably, the biofilm biovolume of ΔpqsA biofilms grown in presence of sub-MIC of tobramycin was significantly reduced (53.6%) when compared to the biovolume of H103 biofilms grown in the same conditions. By contrast, the eDNA relative abundance did not increase in ΔpqsA biofilms in presence of tobramycin compared to biofilms of the same strain without tobramycin, on the opposite to the tobramycin-induced eDNA increase seen in H103 biofilms (Fig. 4e). The relative eDNA abundances were thus not significantly different in tobramycin-free H103 biofilms and ΔpqsA biofilms with or without antibiotic, and were only higher in H103 biofilms with tobramycin (Fig. 4e). Taken together, these data indicate that whereas the biofilm biovolume enhancement could still occur in response to sub-MIC of tobramycin in ΔpqsA biofilms, at least a part of the increase of eDNA release appears to be HAQ-dependent.

Fig. 4
figure4

Tobramycin-enhanced biofilm formation is associated with increased production of QS molecules. a Quantification of the two main AHLs (C4-HSL and 3-oxo-C12-HSL) of Rhl and Las QS systems by LC-MS/MS analysis. Error bars represent standard error of the means (n ≥ 3). b Quantification of HAQ molecules (HHQ, PQS, and HQNO) by LC-MS/MS analysis. Error bars represent standard error of the means (n ≥ 3). c Representative CLSM 3D-top micrographs of 24-h-old biofilms of P. aeruginosa H103 and ΔpqsA mutant strains exposed to tobramycin (0.8 μg ml−1) compared to untreated biofilms. Scale bars = 20 µm. CLSM images were analyzed using COMSTAT software to quantify d biofilm biovolumes. Error bars represent standard error of the means (n = 3) and e eDNA relative abundances. Error bars represent standard error of the means (n = 3). eDNA values were normalized to biofilm biovolumes. Asterisks indicate a significant difference as determined by a two-tailed t test: , P = 0.0001 to 0.001; , P = 0.001 to 0.01; , P = 0.01 to 0.05; NS (not significant), P ≥ 0.05

PrrF sRNAs promote tobramycin-enhanced biofilm formation

A previous study reported that biofilm formation in the prrF mutant is not induced under sub-MIC of tobramycin.32 Thus, the effect of tobramycin was assessed on PrrF sRNAs expression using RT-qPCR. Interestingly, the expression of PrrF sRNAs was significantly increased by 2.4-fold (Fig. 5a), suggesting their involvement in the tobramycin-enhanced biofilm formation in P. aeruginosa. To further validate this hypothesis, biofilm formation and eDNA release were evaluated in a ΔprrF mutant under tobramycin exposure (Fig. 5b). As seen in Fig. 5c, no significant difference was observed between the biofilm biovolume of P. aeruginosa ΔprrF mutant and H103 strains in the absence of antibiotic. Remarkably, sub-MIC of tobramycin-enhanced biofilm biovolume in ΔprrF mutant compared to ΔprrF tobramycin-free biofilm as in the case of the biofilm formation of H103 grown without or with tobramycin but in a minor rise proportion (Fig. 5c). However, tobramycin-treated biofilm of ΔprrF mutant did not show increased relative abundance of eDNA (Fig. 5d). Interestingly, HAQs quantification by LC-MS/MS showed that deletion of PrrF sRNAs had no significant effect on the production levels of HHQ, PQS, and HQNO when compared to H103 strain grown in the same conditions (Fig. 5e). Moreover, the HAQs levels in the exposed-tobramycin biofilm of ΔprrF mutant were increased to levels at those of the H103 biofilm treated with tobramycin (Fig. 5e). Altogether, these results indicate a link between PrrF sRNAs and eDNA release probably mediated through an HAQ-independent mechanism in response to sub-MIC of tobramycin.

Fig. 5
figure5

Role of PrrF1/F2 sRNAs in tobramycin-enhanced biofilm formation. a Relative prrF mRNA levels in P. aeruginosa biofilms exposed to tobramycin (brown bars) compared to the relative expression of mRNA levels in the control condition (green bars), after 24 h of growth. Quantifications have been obtained from at least three independent experiments and rpoD was used as a control housekeeping gene. Error bars represent standard error of the means (n = 3). b Representative CLSM 3D micrographs of 24-h-old biofilms P. aeruginosa H103 and ΔprrF mutant strains exposed to tobramycin (0.8 μg ml−1) compared to untreated biofilms. Scale bars = 20 µm. CLSM images were analyzed using COMSTAT software to quantify c biofilm biovolumes. Error bars represent standard error of the means (n = 3) and d eDNA relative abundances. eDNA values are normalized to biofilm biomass. Error bars represent standard error of the means (n = 3). e HAQs levels of the ΔprrF mutant and its isogenic parent strain H103 grown with or without tobramycin supplementation, as determined by LC-MS/MS. Error bars represent standard error of the means (n = 3). Statistics were achieved by a two-tailed t test: , P = 0.001 to 0.01; , P = 0.01 to 0.05; NS (not significant), P ≥ 0.05

Effect of tobramycin on iron uptake systems and oxidative stress response in biofilm

The PrrF1 and PrrF2 sRNAs are key elements of P. aeruginosa iron homeostasis32 and previous studies demonstrated the requirement of iron for induction of biofilm formation in P. aeruginosa by sub-MIC of tobramycin.33 Therefore, the effect of tobramycin was explored on the expression of iron and heme acquisition systems. RT-qPCR analyses indicated increased expression of pvdS encoding the PvdS extracytoplasmic function sigma factor (ECFσ)34 and the pvdH biosynthetic gene by about threefold in response to tobramycin (Fig. 6). Similarly, expression of hasI and phuR, encoding the HasI ECFσ for the Has-dependent heme uptake system and heme/hemoglobin outer membrane receptor PhuR increased in the presence of tobramycin, reflecting the activity of the heme acquisition (Has) and the heme uptake (Phu) systems (Fig. 6). Finally, we assayed the Feo system for the uptake of Fe2+ and showed enhanced expression of feoB encoding the inner membrane permease FeoB (Fig. 6). The enhancement of these iron uptake systems in response to tobramycin reveals a high demand of iron that might lead to oxidative damages. Interestingly, proteomic data analysis showed that the two alkyl hydroperoxide reductases AhpF (PA0140) and AhpB (PA0848) were significantly more abundant in tobramycin-exposed biofilm. Additionally, the protein TrxB (PA0849), a thioredoxin reductase, which protects protein disulfide bonds from oxidation was also induced (Supplementary Table 1; Fig. 3). Collectively, these data suggest a contribution of iron and oxidative stress responses into the tobramycin-enhanced biofilm formation in P. aeruginosa that could be mediated by the PrrF sRNAs.

Fig. 6
figure6

Sub-MIC of tobramycin enhance iron/heme uptake strategies in P. aeruginosa biofilm cultures. Relative pvdS, pvdH, hasI, phuR, and feoB mRNA levels in P. aeruginosa biofilm cultures exposed to sub-MIC of tobramycin (green bars) compared to the relative mRNA levels in the control condition (brown bars), after 24 h of growth. Quantifications have been obtained from at least three independent experiments and rpoD was used as a control housekeeping gene. Error bars represent standard error of the means (n = 3). Statistics were achieved by a two-tailed t test: , P = 0.0001 to 0.001; , P = 0.001 to 0.01; , P = 0.01 to 0.05

Discussion

Bacteria have the ability to adapt to numerous environmental stresses by setting up different biological responses such as the enhancement of biofilm formation, notably upon exposure to low antibiotic concentrations.12,13 Through CLSM observations, whole biofilm proteome analysis, gene expression RT-qPCR assays, and phenotypic approaches, we present herein further insights into the adaptation mechanisms leading to increased biofilm formation in P. aeruginosa in response to sub-MIC of tobramycin. The effect of sub-MIC of tobramycin on increased biofilm development in P. aeruginosa was corroborated19,20,21 and the present work demonstrates modifications in the biofilm architecture. Remarkably, tobramycin exposure results in biofilm matrix modifications by increasing eDNA abundance levels, which in turn favors the built up of 3D structures15 leading to elevated biofilm biovolume and thickness, as confirmed by DNase I treatment. This result mirrors those of previous studies that have shown increased matricial extracellular nucleic acids amounts in Enterococcus faecalis and Staphylococcus aureus in response to sub-MICs of ampicillin and methicillin, respectively.35,36

eDNA was previously described to play a structural role in biofilm formation, to bind and shield biofilms from aminoglycosides, and to induce antimicrobial peptide resistance mechanisms in P. aeruginosa.37,38,39,40 The observed rise in eDNA release is presumably a consequence of elevated cell biofilm death that seems to be mediated by a QS-dependent mechanism. Accordingly, data of the current study demonstrate increased production levels of HAQ molecules (HHQ, PQS, and HQNO) in P. aeruginosa H103 strain and decreased eDNA release in ΔpqsA in response to sub-MIC of tobramycin. This finding is in agreement with a previous study which showed that HAQs play a key role in eDNA release, occurring as a result of biofilm subpopulations lysis.28 However, given that ΔpqsA biofilm biovolume decreased, we have been unable to show differences in terms of eDNA release between pqsA mutant and H103 strains in the absence of tobramycin. This result was unexpected and suggests that an alternative potential eDNA-independent mechanism might be involved. Besides, HQNO is a well-known molecule that can act as a cytochrome inhibitor of the respiratory chain,41 inducing thus the production of reactive oxygen species (ROS), which are involved in membrane damages resulting in cell autolysis and eDNA release.42 We found here also that proteins related to phenazine biosynthesis and several extracellular proteases triggered through the QS system are enhanced in presence of sub-MIC tobramycin. Previous findings demonstrated that pyocyanin enhances the matrix stability by interacting with eDNA, thus enabling the strength and development of the biofilm.43,44 Moreover, the current study demonstrated significant higher production levels of the two AHL signal molecules, 3-oxo-C12-HSL and C4-HSL, produced by the Las and Rhl QS systems, respectively, that are involved in P. aeruginosa biofilm development.13,45 The induction of the Las system under tobramycin exposure may trigger the observed increased accumulation of proteins related to HAQ biosynthesis. Altogether these data suggest a key role for the HAQ, including in signaling, and probably also ROS in the release of eDNA leading to increased biofilm development in response to sub-MIC of tobramycin.

Previous studies reported that PQS triggers iron-starvation response in P. aeruginosa by its ability to chelate ferric iron (Fe3+) and functions as an iron trap associated with the outer membrane.46,47 In fact, several iron acquisition systems are overexpressed in P. aeruginosa biofilm under tobramycin exposure. This study demonstrates higher expression levels of genes involved in the biosynthesis of pyoverdine siderophore, which is of importance for biofilm formation.48,49 The two heme uptake systems Has and Phu and the ferrous iron uptake Feo system are also increased. Remarkably, phenazine-1-carboxylic acid, that can reduce ferric iron to its ferrous oxidation state, promotes biofilm formation through the Feo system.50 Thus, these results reveal a contribution of iron uptake strategies in tobramycin-enhanced biofilm formation in P. aeruginosa. These findings are in line with a previous study that demonstrated the role of iron in the induction of biofilm formation in P. aeruginosa by sub-MIC of tobramycin.33 While the potential of iron to stimulate oxidative stress, the proteomic data of this study showed a rise of the AhpF, AhpB-TrxB2 proteins responsible for an antioxidant mechanism activity51 that would help limiting some adverse effects of ROS. In addition, the PqsR (MvfR) transcriptional regulator activated by PQS modulates the expression of genes involved in the oxidative stress response.51

Besides, the iron-starvation response revealed by gene expression data seems to be involved in the increased expression of regulatory PrrF sRNAs that are known to regulate several genes involved in protection from oxidative stress and iron storage.32,52 Remarkably, an important finding of this study was that biofilms formed by ΔprrF in presence of tobramycin contain less eDNA than H103 strain biofilm formed under the same condition, therefore following a similar trend as the ΔpqsA mutant when compared to P. aeruginosa H103 strain under tobramycin exposure. However, while PrrF sRNAs were shown previously to modulate HAQs production under planktonic conditions,53,54 our study that was conducted in biofilms showed that ΔprrF mutant produced HAQs levels similar to those of the wild-type strain grown with or without tobramycin. These data suggest that HAQs production modulation by PrrF sRNAs might not play an important role in H103 strain and studied conditions and point out to the complex regulation of HAQs production. In summary, these data suggest that regulatory PrrF sRNAs are key players mediating eDNA release through possibly another potential HAQ-independent mechanism leading to tobramycin-increased biofilm formation. Furthermore, the whole proteome data show decreased abundances of RNases including RNaseE, RNaseR, and PNPase in the presence of sub-MIC of tobramycin that appears to explain the increased expression of sRNAs. Recent studies indicate that RNases greatly affect biofilm formation by causing sRNAs decay in microorganisms such as P. aeruginosa, Escherichia coli and Salmonella Typhimurium.55,56,57

In addition, numerous metabolic pathways were affected in the whole biofilm proteome exposed to tobramycin. Especially, proteins related to glycolysis, TCA, and denitrification pathways were under-produced, suggesting a metabolic adaptation under biofilm growth in the presence of tobramycin. Interestingly, a recent study reported the functional enrichment of proteins related to TCA, carbon metabolism and energy derivation, and electron transport activities, which were under-accumulated in the presence of tobramycin under planktonic conditions.24 P. aeruginosa was demonstrated to use PQS to downregulate genes involved in denitrification in planktonic conditions,58 indicating a link between QS and energy metabolism. Recently, AHL-mediated QS was shown to alter TCA cycle intermediates, and fatty acid and amino acid metabolism during stationary phase.59 Amino acid metabolism (as carnitine and lysine) was also affected upon tobramycin exposure in our study according to previous data observed when P. aeruginosa was grown in planktonic conditions.24 Moreover, and in line with our results, the enhanced catabolism of the amino acids arginine, phenylalanine and tyrosine was reported.60

Overall, we suggest herein new potential adaptive mechanisms on how sublethal concentrations of tobramycin lead to increased biofilm formation in P. aeruginosa. Importantly, the release of eDNA might explain, at least in part, the enhancement of biofilm formation and point to the fundamental role of the biofilm matrix. HAQs and regulatory PrrF sRNAs appears to be key players in the eDNA release since no effect of tobramycin was observed on eDNA release in ΔpqsA and ΔprrF mutants. However, there was still an impact of tobramycin on ΔpqsA and ΔprrF biofilm formation suggesting that alternative mechanism(s) may possibly be involved. In addition, it is apparent that the decreased eDNA release observed in ΔpqsA and ΔprrF mutants occur through distinct mechanisms and we cannot disregard the importance of the other discussed adaptive mechanisms which deserve further investigations.

Methods

Bacterial strains, growth conditions and antibiotics

The P. aeruginosa H103 strain and derivatives are listed in Supplementary Table 4. P. aeruginosa H103 biofilms were grown on membrane filters (25 mm diameter, 0.2 µm pore size, Whatman) placed over the surface of freshly prepared LB agar plates supplemented or not with the required concentration of tobramycin (Sigma-Aldrich). To this end, overnight planktonic cultures grown aerobically at 37 °C in LB broth on a rotary shaker (180 r.p.m.) were diluted to an OD at 580 nm of 1 and 100 µl spotted on the membrane. The bacteria were incubated at 37 °C for 24 h on static conditions. The antibiotics stock solutions used in this study were sterilized by filtration through 0.22-µm filters, aliquoted into daily-use volumes and kept at −20 °C.

Sensitivity of P. aeruginosa to tobramycin

ETEST® tobramycin gradient strip (0.016−256 µg ml−1; Biomérieux) was used to assess the MIC assay for P. aeruginosa strain H103 according to the manufacturer’s instructions. An inoculum containing a concentration of bacteria that approximates the 0.5 McFarland turbidity standard was used. Antibiotic sensitivity was read after 24 h incubation at 37 °C.

Construction of the ΔpqsA and ΔprrF mutant strains

The pqsA and prrF mutant strains were constructed by following the procedure described by Quénée et al.61 Briefly, the pqsA and prrF-flanking regions were PCR amplified using the primer pairs listed in Supplementary Table 5. PCR products pqsA- or prrF-upstream and pqsA- or prrF-downstream were digested by SacI/XbaI or EcoRI/XbaI and XbaI/HindIII, respectively, and cloned by a three-way ligation into the suicide vector pEX100Tlink opened by SacI and HindIII or EcoRI and HindIII. These cloning strategies resulted in the construction of pEX:ΔpqsA and pEX:ΔprrF plasmids, respectively. The lox-aacC1-lox cassette encoding gentamicin (Gm) resistance was excised from pUCGmlox61 using XbaI and was subcloned into the unique XbaI site of pEX:ΔpqsA and pEX:ΔprrF. The resulting pEX:ΔpqsA:Gmlox and pEX:ΔprrF:Gmlox plasmids were then introduced into the E. coli donor/helper strain S17.1 and transferred by conjugation into P. aeruginosa H103. Gm-resistant colonies grown on Pseudomonas isolation agar (PIA) plates were counter-selected on 5% sucrose LB agar plates, and the double recombinants were selected for their Gm resistance and carbenicillin (Cb) sensitivity. Finally, the aacC1 gene conferring Gm resistance was excised by the Cre recombinase encoded by pCM157.62 The resulting ΔpqsA and ΔprrF mutant strains were checked by PCR using primer pairs pqsA-SacI-F/pqsA-HindIII-R and prrF-EcoRI-F/prrF-HindIII-R, respectively (Supplementary Table 5), and the resulting fragments were verified by DNA sequencing (Sanger sequencing services, Genewiz).

Confocal laser scanning microscopy (CLSM)

P. aeruginosa H103, ΔpqsA, and ΔprrF biofilms were grown in LB medium supplemented or not with the required concentration of tobramycin on a 24-well glass-bottomed microplates for 24 h at 37 °C in static conditions. Biofilm formation in the presence of DNase I from bovine pancreas (Sigma-Aldrich) was performed by supplementing LB medium with DNase I at 100 µg ml−1.63 Prior to image acquisition, biofilm cells and eDNA matrix component were stained with fluorescent dyes and observed by CLSM. Biofilm cells were stained by adding 5 µM of SYTO® 9 green fluorescent nucleic acid stain (Invitrogen, Thermo Fisher Scientific; excitation at 488 nm and emission from 500 to 550 nm) or 5 µM of SYTO® 62 red fluorescent nucleic acid stain (Molecular Probes, Life Technologies; excitation at 652 nm and emission at 676 nm) prepared in sterile physiological solution (0.9% NaCl), incubated at room temperature for 15 min in the dark and then washed twice with sterile physiological solution (0.9% NaCl).

The eDNA biofilm-component matrix was stained using 1 µM of 7-hydroxy-9H-(1,3-dichloro-9,9-dimethylacridin-2-one) (DDAO), a red fluorescent probe (Molecular Probes, life; excitation at 663 nm and emission at 660 nm).

The Live/Dead fluorescent staining was performed using the LIVE/DEAD® BacLightTM Bacterial Viability Kit (Thermo Fisher Scientific). The cells were labeled with a mixture (v/v) of component A (SYTO 9 dye, 1.67 mM/propidium iodide, 1.67 mM) and component B (SYTO 9 dye, 1.67 mM/propidium iodide, 18.3 mM) according to the manufacturer’s recommendations.

The CLSM observations were carried out with a Zeiss LSM710 microscope (Carl Zeiss Microscopy) using a ×63 oil immersion objective. Images were taken every micrometer throughout the whole biofilm depth. For visualization and processing of 3D images, the Zen 2.1 SP1 zen software (https://www.zeiss.com/microscopy/int/downloads/zen.html) (Carl Zeiss Microscopy) was used. The thicknesses (μm) and biovolumes (μm3 μm−2) of the biofilms were measured using the COMSTAT2 software (http://www.imageanalysis.dk/).64 At least three image stacks from each of three independent experiments were used for each analysis.

Reverse transcription-quantitative PCR analysis (RT-qPCR)

Total RNAs from three independent biofilm cultures were isolated by the hot acid-phenol method,65 followed by treatment with Turbo DNA-freeTM kit (Invitrogen) according to the manufacturer’s protocol. Synthesis of cDNAs and RT-qPCR was achieved as previously described,66 using the oligonucleotides listed in Supplementary Table 3. The mRNAs and sRNAs levels were calculated by comparing the threshold cycles (Ct) of target genes with those of control sample groups and the relative quantification was measured using the 2−ΔΔCt method67 using DataAssistTM software (Applied Biosystems).

LTQ-orbitrap analysis

The sample preparation, protein digestion, tandem mass spectrometry and whole proteome analysis was performed as previously described.68 All experiments were performed on an LTQ-Orbitrap Elite (Thermo Scientific) coupled to an Easy nLC II system (Thermo Scientific). One microliter of sample was injected onto an enrichment column (C18 PepMap100, Thermo Scientific). The separation was performed with an analytical column needle (NTCC-360/100-5-153, NikkyoTechnos, Japan). The mobile phase consisted of H2O/0.1 % formic acid (FA) (buffer A) and CH3CN/FA 0.1 % (buffer B). Tryptic peptides were eluted at a flow rate of 300 nl/min using a three-step linear gradient: from 2 to 40% B over 75 min, from 40 to 80% B in 4 min and 11 min at 80% B. The mass spectrometer was operated in positive ionization mode with capillary voltage and source temperature set at 1.5 kV and 275 °C, respectively. The samples were analyzed using CID (collision induced dissociation) method. The first scan (MS spectra) was recorded in the Orbitrap analyzer (R = 60,000) with the mass range m/z 400–1800. Then, the 20 most intense ions were selected for MS2 experiments. Singly charged species were excluded for MS2 experiments. Dynamic exclusion of already fragmented precursor ions was applied for 30 s, with a repeat count of 1, a repeat duration of 30 s and an exclusion mass width of ±10 ppm. Fragmentation occurred in the linear ion trap analyzer with collision energy of 35%. All measurements in the Orbitrap analyzer were performed with on-the-fly internal recalibration (lock mass) at m/z 445.12002 (polydimethylcyclosiloxane). After MS analysis, raw data were imported in Progenesis LC-MS software (Nonlinear Dynamics). For comparison, one sample was set as a reference and the retention times of all other samples within the experiment were aligned. After alignment and normalization, statistical analysis was performed for one-way analysis of variance (ANOVA) calculations. Peptide features presenting a p value and a q value less than 0.05, and a power greater than 0.8 were retained. MS/MS spectra from selected peptides were exported for peptide identification with Mascot (Matrix Science) against the database restricted to P. aeruginosa PAO1 (http://www.pseudomonas.com).26 Database searches were performed with the following parameters: 1 missed trypsin cleavage site allowed; variable modifications: carbamidomethylation of cysteine and oxidation of methionine. Peptides with scores above 20 were imported into Progenesis. For each condition, the total cumulative abundance of the protein was calculated by summing the abundances of peptides. Proteins identified with less than two peptides were discarded. Only the proteins that varied by twofold in these average normalized abundances between growth conditions were retained. Expression data for all significantly differentially produced proteins are available in Supplementary Tables 1 and 2.

Functional enrichment of proteomic data

The enrichment factor (EF) was calculated using the following formula: EF = (number of specific PseudoCAP classes detected/number of all PseudoCAP classes detected)/ (number of specific PseudoCAP classes annotated/number of all PseudoCAP classes annotated). Functional categories displaying an EF ≥ 1.5 are defined as overrepresented in the functional proteomic profiling of the tobramycin-exposed biofilm (Supplementary Fig. 1).

P. aeruginosa whole biofilm Protein−Protein Interaction Network (PPIN) inference

P. aeruginosa PAO1 Protein−Protein Interaction Network (PPIN) was retrieved from the STRING database (http://string-db.org/).69 One hundred and ninety-one functional connections were inferred between 111 proteins of the 174 proteins by selecting connections over a threshold of 0.7 of confidence combined score. The 63 proteins without any connection to other proteins in the network were removed. The resulting string network was visualized within Cytoscape (version 3.2.1) (http://www.cytoscape.org).27

Extraction and quantification of AHLs and HAQs

Colony biofilms of H103 strain and its derivative mutants exposed or not to tobramycin were resuspended in 0.9% NaCl (three-colony biofilms per 10 ml of 0.9% NaCl). Biofilm suspensions were vortexed for 2 min and the AHL and HAQ molecules were extracted following the technique described in a previous study.70 AHLs and HAQs were quantified by liquid chromatography coupled to mass spectrometry (LC-MS/MS).29,71 The obtained data were normalized to OD of biofilm suspensions. AHL standards were obtained from Sigma [N-butanoyl-l-homoserine lactone (C4-HSL) and N-3-oxododecanoyl-l-homoserine lactone (3-oxo-C12-HSL)].

Statistical analysis

Statistical significance was evaluated using Prism GraphPad online tool (https://www.graphpad.com/quickcalcs/ttest1/). The data were statistically analyzed using unpaired (two sample) two-tailed t test to calculate p values. The mean with standard error of the mean (SEM) were calculated and plotted.

Reporting summary

Further information on experimental design is available in the Nature Research Reporting Summary linked to this paper.

Data availability

The authors declare that all relevant data supporting the findings of the study are available in this article and its Supplementary Information files, or from the corresponding author upon request.

References

  1. 1.

    López, D., Vlamakis, H. & Kolter, R. Biofilms. Cold Spring Harb. Perspect. Biol. 2, a00398 (2010).

    Article  Google Scholar 

  2. 2.

    Hall-Stoodley, L., Costerton, J. W. & Stoodley, P. Bacterial biofilms: from the natural environment to infectious diseases. Nat. Rev. Microbiol. 2, 95–108 (2004).

    CAS  Article  Google Scholar 

  3. 3.

    Flemming, H. C. et al. Biofilms: an emergent form of bacterial life. Nat. Rev. Microbiol. 14, 563–575 (2016).

    CAS  Article  Google Scholar 

  4. 4.

    Ciofu, O., Rojo-Molinero, E., Macià, M. D. & Oliver, A. Antibiotic treatment of biofilm infections. APMIS 125, 304–319 (2017).

    Article  Google Scholar 

  5. 5.

    Kaplan, J. B. Antibiotic-induced biofilm formation. Int. J. Artif. Organs 34, 737–751 (2011).

    CAS  Article  Google Scholar 

  6. 6.

    Tolker-Nielsen, T. Biofilm development. Microbiol. Spectr. 3, MB-0001–MB-2014 (2015).

    Article  Google Scholar 

  7. 7.

    Chevalier, S. et al. Structure, function and regulation of Pseudomonas aeruginosa porins. FEMS Microbiol. Rev. 41, 698–722 (2017).

    CAS  Article  Google Scholar 

  8. 8.

    Lesouhaitier, O. et al. Host peptidic hormones affecting bacterial biofilm formation and virulence. J. Innate Immun. 5, 1–15 (2018).

    Google Scholar 

  9. 9.

    Davies, J., Spiegelman, G. B. & Yim, G. The world of subinhibitory antibiotic concentrations. Curr. Opin. Microbiol. 9, 445–453 (2006).

    CAS  Article  Google Scholar 

  10. 10.

    Fajardo, A. & Martínez, J. L. Antibiotics as signals that trigger specific bacterial responses. Curr. Opin. Microbiol. 11, 161–167 (2008).

    CAS  Article  Google Scholar 

  11. 11.

    Song, T., Duperthuy, M. & Wai, S. Sub-optimal treatment of bacterial biofilms. Antibiotics 5, 23 (2016).

    Article  Google Scholar 

  12. 12.

    Andersson, D. I. & Hughes, D. Microbiological effects of sublethal levels of antibiotics. Nat. Rev. Microbiol. 12, 465–478 (2014).

    CAS  Article  Google Scholar 

  13. 13.

    Moradali, M. F., Ghods, S. & Rehm, B. H. A. Pseudomonas aeruginosa lifestyle: a paradigm for adaptation, survival, and persistence. Front. Cell. Infect. Microbiol. 7, 39 (2017).

    Article  Google Scholar 

  14. 14.

    Flemming, H.-C. & Wingender, J. The biofilm matrix. Nat. Rev. Microbiol. 8, 623–633 (2010).

    CAS  Article  Google Scholar 

  15. 15.

    Mann, E. E. & Wozniak, D. J. Pseudomonas biofilm matrix composition and niche biology. FEMS Microbiol. Rev. 36, 893–916 (2012).

    CAS  Article  Google Scholar 

  16. 16.

    Gellatly, S. L. & Hancock, R. E. W. Pseudomonas aeruginosa: new insights into pathogenesis and host defenses. Pathog. Dis. 67, 159–173 (2013).

    CAS  Article  Google Scholar 

  17. 17.

    Sousa, A. & Pereira, M. Pseudomonas aeruginosa diversification during infection development in cystic fibrosis lungs—a review. Pathogens 3, 680–703 (2014).

    Article  Google Scholar 

  18. 18.

    Cheer, S. M., Waugh, J. & Noble, S. Inhaled tobramycin (TOBI®): a review of its use in the management of Pseudomonas aeruginosa infections in patients with cystic fibrosis. Drugs 63, 2501–2520 (2003).

    CAS  Article  Google Scholar 

  19. 19.

    Hoffman, L. R. et al. Aminoglycoside antibiotics induce bacterial biofilm formation. Nature 436, 1171–1175 (2005).

    CAS  Article  Google Scholar 

  20. 20.

    Jones, C., Allsopp, L., Horlick, J., Kulasekara, H. & Filloux, A. Subinhibitory concentration of kanamycin induces the Pseudomonas aeruginosa type VI secretion system. PLoS ONE 8, e81132 (2013).

    CAS  Article  Google Scholar 

  21. 21.

    Linares, J. F., Gustafsson, I., Baquero, F. & Martinez, J. L. Antibiotics as intermicrobial signaling agents instead of weapons. Proc. Natl Acad. Sci. USA 103, 19484–19489 (2006).

    CAS  Article  Google Scholar 

  22. 22.

    Elliott, D., Burns, J. L. & Hoffman, L. R. Exploratory study of the prevalence and clinical significance of tobramycin-mediated biofilm induction in Pseudomonas aeruginosa isolates from cystic fibrosis patients. Antimicrob. Agents Chemother. 54, 3024–3026 (2010).

    CAS  Article  Google Scholar 

  23. 23.

    Gotoh, H. et al. Pseudomonas aeruginosa, under DNA replication inhibition, tends to form biofilms via Arr. Res. Microbiol. 159, 294–302 (2008).

    CAS  Article  Google Scholar 

  24. 24.

    Wu, X. et al. Dynamic proteome response of Pseudomonas aeruginosa to tobramycin antibiotic treatment. Mol. Cell. Proteom. 14, 2126–2137 (2015).

    CAS  Article  Google Scholar 

  25. 25.

    Whitchurch, C. B., Tolker-Nielsen, T., Ragas, P. C. & Mattick, J. S. Extracellular DNA required for bacterial biofilm formation. Science 295, 1487 (2002).

    CAS  Article  Google Scholar 

  26. 26.

    Winsor, G. L. et al. Enhanced annotations and features for comparing thousands of Pseudomonas genomes in the Pseudomonas genome database. Nucleic Acids Res. 44, D646–D653 (2016).

    CAS  Article  Google Scholar 

  27. 27.

    Shannon, P. et al. Cytoscape: a software environment for integrated models of biomolecular interaction networks. Genome Res. 13, 2498–2504 (2003).

    CAS  Article  Google Scholar 

  28. 28.

    Allesen‐Holm, M. et al. A characterization of DNA release in Pseudomonas aeruginosa cultures and biofilms. Mol. Microbiol. 59, 1114–1128 (2006).

    Article  Google Scholar 

  29. 29.

    Déziel, E. et al. Analysis of Pseudomonas aeruginosa 4-hydroxy-2-alkylquinolines (HAQs) reveals a role for 4-hydroxy-2-heptylquinoline in cell-to-cell communication. Proc. Natl Acad. Sci. USA 101, 1339–1344 (2004).

    Article  Google Scholar 

  30. 30.

    Schertzer, J. W., Brown, S. A. & Whiteley, M. Oxygen levels rapidly modulate Pseudomonas aeruginosa social behaviours via substrate limitation of PqsH. Mol. Microbiol. 77, 1527–1538 (2010).

    CAS  Article  Google Scholar 

  31. 31.

    Lépine, F., Milot, S., Déziel, E., He, J. & Rahme, L. G. Electrospray/mass spectrometric identification and analysis of 4-hydroxy-2-alkylquinolines (HAQs) produced by Pseudomonas aeruginosa. J. Am. Soc. Mass Spectrom. 15, 862–869 (2004).

    Article  Google Scholar 

  32. 32.

    Reinhart, A. A. et al. The prrF-encoded small regulatory RNAs are required for iron homeostasis and virulence of Pseudomonas aeruginosa. Infect. Immun. 83, 863–875 (2015).

    Article  Google Scholar 

  33. 33.

    Oglesby-Sherrouse, A. G., Djapgne, L., Nguyen, A. T., Vasil, A. I. & Vasil, M. L. The complex interplay of iron, biofilm formation, and mucoidy affecting antimicrobial resistance of Pseudomonas aeruginosa. Pathog. Dis. 70, 307–320 (2014).

    CAS  Article  Google Scholar 

  34. 34.

    Chevalier, S. et al. Extracytoplasmic function sigma factors in Pseudomonas aeruginosa. Biochim. Biophys. Acta—Gene Regul. Mech. 17, 30313–30319 (2018).

    Google Scholar 

  35. 35.

    Kaplan, J. B. et al. Low levels of β-lactam antibiotics induce extracellular DNA release and biofilm formation in Staphylococcus aureus. mBio 3, e00198–12 (2012).

    Article  Google Scholar 

  36. 36.

    Yu, W., Hallinen, K. M. & Wood, K. B. Interplay between antibiotic efficacy and drug-induced lysis underlies enhanced biofilm formation at subinhibitory drug concentrations. Antimicrob. Agents Chemother. 62, e01603–e01617 (2018).

    PubMed  Google Scholar 

  37. 37.

    Mulcahy, H., Charron-Mazenod, L. & Lewenza, S. Extracellular DNA chelates cations and induces antibiotic resistance in Pseudomonas aeruginosa biofilms. PLoS Pathog. 4, e1000213 (2008).

    Article  Google Scholar 

  38. 38.

    Lewenza, S. Extracellular DNA-induced antimicrobial peptide resistance mechanisms in Pseudomonas aeruginosa. Front. Microbiol. 4, 21 (2013).

    Article  Google Scholar 

  39. 39.

    Chiang, W.-C. et al. Extracellular DNA shields against aminoglycosides in Pseudomonas aeruginosa biofilms. Antimicrob. Agents Chemother. 57, 2352–2361 (2013).

    CAS  Article  Google Scholar 

  40. 40.

    Wilton, M., Charron-Mazenod, L., Moore, R. & Lewenza, S. Extracellular DNA acidifies biofilms and induces aminoglycoside resistance in Pseudomonas aeruginosa. Antimicrob. Agents Chemother. 60, 544–553 (2016).

    CAS  Article  Google Scholar 

  41. 41.

    Voggu, L. et al. Microevolution of cytochrome bd oxidase in staphylococci and its implication in resistance to respiratory toxins released by. Pseudomonas. J. Bacteriol. 188, 8079–8086 (2006).

    CAS  Article  Google Scholar 

  42. 42.

    Hazan, R. et al. Auto poisoning of the respiratory chain by a quorum-sensing-regulated molecule favors biofilm formation and antibiotic tolerance. Curr. Biol. 26, 195–206 (2016).

    CAS  Article  Google Scholar 

  43. 43.

    Das, T. & Manefield, M. Pyocyanin promotes extracellular DNA release in Pseudomonas aeruginosa. PLoS ONE 7, e46718 (2012).

    CAS  Article  Google Scholar 

  44. 44.

    Das, T., Sehar, S. & Manefield, M. The roles of extracellular DNA in the structural integrity of extracellular polymeric substance and bacterial biofilm development. Environ. Microbiol. Rep. 5, 778–786 (2013).

    CAS  Article  Google Scholar 

  45. 45.

    Williams, P. & Cámara, M. Quorum sensing and environmental adaptation in Pseudomonas aeruginosa: a tale of regulatory networks and multifunctional signal molecules. Curr. Opin. Microbiol. 12, 182–191 (2009).

    CAS  Article  Google Scholar 

  46. 46.

    Bredenbruch, F., Geffers, R., Nimtz, M., Buer, J. & Häussler, S. The Pseudomonas aeruginosa quinolone signal (PQS) has an iron-chelating activity. Environ. Microbiol. 8, 1318–1329 (2006).

    CAS  Article  Google Scholar 

  47. 47.

    Diggle, S. P. et al. The Pseudomonas aeruginosa 4-quinolone signal molecules HHQ and PQS play multifunctional roles in quorum sensing and iron entrapment. Chem. Biol. 14, 87–96 (2007).

    CAS  Article  Google Scholar 

  48. 48.

    Cornelis, P., Matthijs, S. & Van Oeffelen, L. Iron uptake regulation in Pseudomonas aeruginosa. Biometals 22, 15–22 (2009).

    CAS  Article  Google Scholar 

  49. 49.

    Cornelis, P. & Dingemans, J. Pseudomonas aeruginosa adapts its iron uptake strategies in function of the type of infections. Front. Cell. Infect. Microbiol. 3, 75 (2013).

    Article  Google Scholar 

  50. 50.

    Wang, Y. et al. Phenazine-1-carboxylic acid promotes bacterial biofilm development via ferrous iron acquisition. J. Bacteriol. 193, 3606–3617 (2011).

    CAS  Article  Google Scholar 

  51. 51.

    Maura, D., Hazan, R., Kitao, T., Ballok, A. E. & Rahme, L. G. Evidence for direct control of virulence and defense gene circuits by the Pseudomonas aeruginosa quorum sensing regulator, MvfR. Sci. Rep. 6, 34083 (2016).

    CAS  Article  Google Scholar 

  52. 52.

    Reinhart, A. A. et al. The Pseudomonas aeruginosa PrrF small RNAs regulate iron homeostasis during acute murine lung infection. Infect. Immun. 85, e00764–16 (2017).

    CAS  Article  Google Scholar 

  53. 53.

    Djapgne, L. et al. The Pseudomonas aeruginosa PrrF1 and PrrF2 small regulatory RNAs (sRNAs) promote 2-alkyl-4-quinolone production through redundant regulation of the antR mRNA. J. Bacteriol. 200, e00704–e00717 (2018).

    CAS  Article  Google Scholar 

  54. 54.

    Oglesby, A. G. et al. The influence of iron on Pseudomonas aeruginosa physiology: A regulatory link between iron and quorum sensing. J. Biol. Chem. 283, 15558–15567 (2008).

    CAS  Article  Google Scholar 

  55. 55.

    Barria, C., Vania, P., Bravo, A. M. & Cecilia, M. A. Ribonucleases as modulators of bacterial stress response. In Stress and Environmental Regulation of Gene Expression and Adaptation in Bacteria 1st edn, (ed. de Bruijn, F. J.) Vol. 1. (John Wiley & Sons, Inc., Hoboken, New Jersey, 2016).

  56. 56.

    Saramago, M. et al. The role of RNases in the regulation of small RNAs. Curr. Opin. Microbiol. 18, 105–115 (2014).

    CAS  Article  Google Scholar 

  57. 57.

    Pobre, V. & Arraiano, C. M. Next generation sequencing analysis reveals that the ribonucleases RNase II, RNase R and PNPase affect bacterial motility and biofilm formation in E. coli. BMC Genom. 16, 72 (2015).

    Article  Google Scholar 

  58. 58.

    Rampioni, G. et al. Unravelling the genome-wide contributions of specific 2-alkyl-4-quinolones and PqsE to quorum sensing in Pseudomonas aeruginosa. PLoS Pathog. 12, e1006029 (2016).

    Article  Google Scholar 

  59. 59.

    Davenport, P. W., Griffin, J. L. & Welch, M. Quorum sensing is accompanied by global metabolic changes in the opportunistic human pathogen Pseudomonas aeruginosa. J. Bacteriol. 197, 2072–2082 (2015).

    CAS  Article  Google Scholar 

  60. 60.

    Bernier, S. P., Ha, D.-G., Khan, W., Merritt, J. H. & O’Toole, G. A. Modulation of Pseudomonas aeruginosa surface-associated group behaviors by individual amino acids through c-di-GMP signaling. Res. Microbiol. 162, 680–688 (2011).

    CAS  Article  Google Scholar 

  61. 61.

    Quénée, L., Lamotte, D. & Polack, B. Combined sacB-based negative selection and cre-lox antibiotic marker recycling for efficient gene deletion in Pseudomonas aeruginosa. BioTechniques 38, 63–67 (2005).

    Article  Google Scholar 

  62. 62.

    Marx, C. J. & Lidstrom, M. E. Broad-host-range cre-lox system for antibiotic marker recycling in Gram-negative bacteria. BioTechniques 33, 1062–1067 (2002).

    CAS  Article  Google Scholar 

  63. 63.

    Tetz, V. V. & Tetz, G. V. Effect of extracellular DNA destruction by DNase I on characteristics of forming biofilms. DNA Cell Biol. 8, 399–405 (2010).

    Article  Google Scholar 

  64. 64.

    Heydorn, A. et al. Quantification of biofilm structures by the novel computer program COMSTAT. Microbiology 146, 2395–2407 (2000).

    CAS  Article  Google Scholar 

  65. 65.

    Bouffartigues, E. et al. Transcription of the oprF gene of Pseudomonas aeruginosa is dependent mainly on the sigX sigma factor and is sucrose induced. J. Bacteriol. 194, 4301–4311 (2012).

    CAS  Article  Google Scholar 

  66. 66.

    Bouffartigues, E. et al. The absence of the Pseudomonas aeruginosa OprF protein leads to increased biofilm formation through variation in c-di-GMP level. Front. Microbiol. 6, 630 (2015).

    Article  Google Scholar 

  67. 67.

    Pfaffl, M. W. A new mathematical model for relative quantification in real-time RT-PCR. Nucleic Acids Res. 29, e45 (2001).

    CAS  Article  Google Scholar 

  68. 68.

    Clamens, T. et al. The aliphatic amidase AmiE is involved in regulation of Pseudomonas aeruginosa virulence. Sci. Rep. 7, 41178 (2017).

    CAS  Article  Google Scholar 

  69. 69.

    Szklarczyk, D. et al. The STRING database in 2017: quality-controlled protein–protein association networks, made broadly accessible. Nucleic Acids Res. 45, D362–D368 (2017).

    CAS  Article  Google Scholar 

  70. 70.

    Tahrioui, A., Quesada, E. & Llamas, I. The hanR/hanl quorum-sensing system of Halomonas anticariensis, a moderately halophilic bacterium. Microbiology 157, 3378–3387 (2011).

    CAS  Article  Google Scholar 

  71. 71.

    Bazire, A. et al. Osmotic stress and phosphate limitation alter production of cell-to-cell signal molecules and rhamnolipid biosurfactant by Pseudomonas aeruginosa. FEMS Microbiol. Lett. 253, 125–131 (2005).

    CAS  Article  Google Scholar 

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Acknowledgements

The LMSM is supported by the Région Normandie (France), Evreux Portes de Normandie (France), European FEDER funds and the French Association “Vaincre la Mucoviscidose”. A.T. is supported by a post-doctoral fellowship from European Union (FEDER) and Région Normandie (France). D.T. and R.D. were supported by doctoral fellowships from the Région Normandie (France). The funders had no role in study design, data collection and interpretation, or the decision to submit this work for publication.

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A.T., S.C., E.B., and O.L. designed the experiments. A.T., R.D., E.B., S.R., J.H., O.M., D.T., L.T, and M.-C.G. conducted experiments and analyzed the data. A.T., S.C., P.C., E.B., A.D., E.D., G.B.-W., M.F., and N.O. contributed to the writing of the manuscript.

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Correspondence to Ali Tahrioui.

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Tahrioui, A., Duchesne, R., Bouffartigues, E. et al. Extracellular DNA release, quorum sensing, and PrrF1/F2 small RNAs are key players in Pseudomonas aeruginosa tobramycin-enhanced biofilm formation. npj Biofilms Microbiomes 5, 15 (2019). https://doi.org/10.1038/s41522-019-0088-3

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