Search tips
Search criteria 


Logo of aemPermissionsJournals.ASM.orgJournalAEM ArticleJournal InfoAuthorsReviewers
Appl Environ Microbiol. 2012 August; 78(15): 5060–5069.
PMCID: PMC3416407

Fluorescence-Based Reporter for Gauging Cyclic Di-GMP Levels in Pseudomonas aeruginosa


The increased tolerance toward the host immune system and antibiotics displayed by biofilm-forming Pseudomonas aeruginosa and other bacteria in chronic infections such as cystic fibrosis bronchopneumonia is of major concern. Targeting of biofilm formation is believed to be a key aspect in the development of novel antipathogenic drugs that can augment the effect of classic antibiotics by decreasing antimicrobial tolerance. The second messenger cyclic di-GMP is a positive regulator of biofilm formation, and cyclic di-GMP signaling is now regarded as a potential target for the development of antipathogenic compounds. Here we describe the development of fluorescent monitors that can gauge the cellular level of cyclic di-GMP in P. aeruginosa. We have created cyclic di-GMP level reporters by transcriptionally fusing the cyclic di-GMP-responsive cdrA promoter to genes encoding green fluorescent protein. We show that the reporter constructs give a fluorescent readout of the intracellular level of cyclic di-GMP in P. aeruginosa strains with different levels of cyclic di-GMP. Furthermore, we show that the reporters are able to detect increased turnover of cyclic di-GMP mediated by treatment of P. aeruginosa with the phosphodiesterase inducer nitric oxide. Considering that biofilm formation is a necessity for the subsequent development of a chronic infection and therefore a pathogenicity trait, the reporters display a significant potential for use in the identification of novel antipathogenic compounds targeting cyclic di-GMP signaling, as well as for use in research aiming at understanding the biofilm biology of P. aeruginosa.


Biofilm-forming bacteria are increasingly recognized as a serious problem in a variety of settings, from fouling of pipelines to infections of humans. Biofilms display increased tolerance toward antibiotics and the host immune system, which makes infections caused by them difficult if not impossible to eradicate (14). This inadequacy of antibiotics has led researchers to look into new strategies for combating biofilm-based infections. One such strategy is the development of antipathogenic drugs (19). The idea behind this strategy is to identify molecular targets that are important to the pathogenicity of the bacteria and to develop drugs that interfere with the actions of the target. Interference with these targets should render the bacteria more susceptible to the action of the immune system and/or antibiotics. The drugs that are developed should not affect growth of the bacteria, making resistance less likely to develop, since no direct selective pressure is exerted by the compounds.

The antipathogenic drug principle has been tested with the opportunistic pathogenic bacterium Pseudomonas aeruginosa as a model organism, and proof of concept has been delivered (21). This common environmental bacterium exploits weaknesses in immunocompromised individuals and people with cystic fibrosis (CF) to establish infections. In the latter case, the bacterium enters the lungs and establishes a recalcitrant and terminal infection that responds poorly to the actions of the immune system and antibiotic treatment regimens (reviewed in reference 27). This recalcitrance is believed to be a consequence of the bacteria residing in biofilms, which have been shown to shield them from the immune system and increase their tolerance toward antibiotics (1, 7). The biofilm-forming capability resulting in immune system evasion and antibiotic tolerance should therefore be recognized as a key target in the development of antipathogenic drugs against P. aeruginosa.

Protection from the immune system is thought to occur due to production of biofilm extracellular matrix components (35) and rhamnolipid, a cytolytic surfactant (1, 28). Rhamnolipid and the increased antibiotic tolerance, together with production of other virulence factors imposing damage to the infected tissue, have been shown to be quorum sensing dependent. Consequently, there has been substantial research within the field of developing antipathogenic drugs targeted against the LuxR-type quorum-sensing regulator LasR of P. aeruginosa (8). Screening for these quorum-sensing inhibitors has been aided by the development of genetic tools allowing monitoring of quorum-sensing activity with the aim of identifying compounds that interfere with the quorum-sensing regulators. Fluorescent reporters constructed as quorum-sensing-regulated promoters transcriptionally fused to gfp have especially been of great value in the work and have led to identification of potent inhibitors such as brominated furanones and the fungal secondary products penicillic acid and patulin (20, 21, 40).

Besides quorum sensing, another interesting signaling system, based on the secondary messenger cyclic di-GMP (c-di-GMP), which controls important events in the biofilm developmental life cycle in P. aeruginosa and many other bacteria, has recently come to the forefront. The messenger is synthesized by diguanylate cyclases (DGCs) with a characteristic GGDEF domain (42) and degraded by phosphodiesterases (PDEs) with characteristic EAL or HD-GYP domains (41, 43). c-di-GMP transmits a wealth of environmental signals through various effector proteins to positively control biofilm-promoting exopolysaccharide and adhesin expression (9, 15, 17, 24, 34, 45), as well as negatively control flagellum- and type IV pilus-driven motility (23, 29, 36). Evidence has been provided that maintenance of a low level of c-di-GMP prevents biofilm formation and that provoked decreases in the intracellular level of c-di-GMP can induce dispersal of already established biofilms (e.g., see reference 18). These findings suggest that antipathogenic drugs targeting c-di-GMP signaling may be developed either to prevent biofilms from forming during infections or to disperse already established biofilms, making them susceptible to efficient treatment by coadministration of classic antibiotics that show much more potential against planktonic bacteria. A decrease in c-di-GMP levels may be achieved through inhibition of DGCs or activation of PDEs (e.g., see reference 6). Furthermore, signaling could be disrupted by inhibiting the activity of effector proteins without changing the c-di-GMP level itself.

To efficiently screen for antipathogenic drug candidates that target c-di-GMP metabolism, a valuable tool would be a reporter of the intracellular levels of c-di-GMP that functions in a manner similar to that of the previously mentioned monitors of quorum sensing. We have created two series of c-di-GMP reporters by transcriptionally fusing a c-di-GMP-responsive promoter to genes encoding green fluorescent protein (GFP). Although the two reporter series were independently constructed, one at the University of Copenhagen, Copenhagen, Denmark, and the other at the University of Washington, Seattle, WA, we publish the information about them jointly in this paper. We show that the reporter constructs are able to provide a fluorescent readout of the intracellular level of c-di-GMP in P. aeruginosa, distinguishing strains with different levels of c-di-GMP. Furthermore, we show that the reporters are able to identify compounds that reduce the intracellular level of c-di-GMP in P. aeruginosa.


Bacterial strains and growth conditions.

The strains and plasmids used in the study are listed in Table 1. Escherichia coli strains were routinely grown in LB medium and on LB agar at 37°C. P. aeruginosa strains were grown in LB medium or ABTG+casA minimal medium (AB medium of Clark and Maaløe [12] supplemented with 2.5 mg thiamine liter−1, 0.5% [wt/vol] glucose and 0.5% [wt/vol] Casamino Acids) and on LB agar or ABTC agar (AB medium supplemented with 2.5 mg thiamine liter−1 and 10 mM citrate) at 37°C. For the c-di-GMP measurements, P. aeruginosa strains were grown in VBMM (25). Antibiotics were supplied where necessary at the following concentrations: for E. coli, 100 μg ampicillin ml−1, 15 μg gentamicin ml−1, 35 μg kanamycin ml−1, and 6 μg chloramphenicol ml−1; for P. aeruginosa, 60 μg gentamicin ml−1 and 200 μg carbenicillin ml−1.

Table 1
Strains and plasmids used in the studya

Construction of Copenhagen c-di-GMP reporter plasmids.

Construction of reporter plasmids was conducted using standard molecular cloning techniques and the E. coli cloning strain DH5α. The cdrA (PA4625) promoter from P. aeruginosa PAO1 was amplified using the primers P-cdrA-up-XbaI and P-cdrA-dn-RBSII-SphI (sequences are available upon request), with the latter including the sequence for an optimized ribosomal binding site (RBSII). The amplified promoter was inserted between the XbaI and SphI sites in the empty expression vector pJBA23, creating plasmid pRYB1. The sequences coding for stable GFP (gfp) and unstable GFP [gfp(ASV), where ASV refers to a peptide tail as described in reference 2] were excised from plasmids pJBA25 and pJBA113, respectively, using SphI and HindIII digestion and inserted between the corresponding sites in pRYB1, creating pRYB1gfp and pRYB1gfp(ASV). The plasmids were sequenced using primers P-cdrA-fwd, P-cdrA-rev, Gfp-seq-int(+), and Gfp-seq-int(−) to ensure that no mutations were found in the cdrA promoter, the ribosomal binding site, or the GFP genes. To create the final P. aeruginosa-compatible reporter plasmids, the reporter cassettes from pRYB1gfp and pRYB1gfp(ASV) were excised using NotI digestion and inserted in NotI-digested pUCP22-Not and pBK-miniTn7-ΩGm, creating pCdrA::gfpC/pCdrA::gfp(ASV)C and pTn7CdrA::gfpC/pTn7CdrA::gfp(ASV)C (where C represents Copenhagen), respectively. Clones were analyzed by XbaI and BglII restriction analysis to select plasmids that harbored the cdrA promoter in the opposite direction than the inherent lac promoter found on pUCP22-Not and pBK-miniTn7-ΩGm (pUC19 derived).

Construction of Seattle c-di-GMP reporter plasmids.

Standard molecular cloning techniques were used in the construction of reporter plasmids in E. coli strain DH5α. The plasmid-based reporters pCdrA::gfpS and pCdrA::gfp(ASV)S (where S represents Seattle) were constructed by amplifying a region comprising 381 bp upstream of the cdrA start codon and 22 bp of the coding sequence using primers PA4625 reporter up and PA4625 reporter down and inserting it into the BamHI sites of the promoterless GFP expression vectors pMH487 and pMH489, respectively. The correct orientation was verified by PCR.

pMH487 and pMH489 were created by inserting an RNase III splice site in XbaI- and SphI-doubly digested pMH305 and pMH391 (20), respectively. The insertion deleted an RBS site lying directly upstream of gfp in the two vectors. pMH305 was created by inserting a NotI-digested RBSII-gfp(Mut3)-T0-T1 fragment from pJBA25 into NotI-digested pUCP22NotI.

Construction of ΔpelΔpsl and ΔwspFΔpelΔpsl background strains.

The pelA, pslBCD, and wspF deletions made in P. aeruginosa PAO1 to create the background strains for the c-di-GMP reporters were conducted as follows. For the pelA and pslBCD deletions, the deletion vectors pMPELA and pMPSL-KO1, respectively, were used. The plasmids were introduced into P. aeruginosa PAO1 and derivatives through triparental mating using pRK600 as a helper plasmid to facilitate the conjugal transfer of the plasmids. Conjugants displaying double-crossover events creating the desired gene deletion were directly selected for by plating of conjugation mixtures on ABTC agar plates supplemented with 5% (wt/vol) sucrose and gentamicin. Deletions were verified by colony PCR using the primer pairs pelA-excis-Up/pelA-excis-Dn and pslBCD-Up/pslBCD-Dn for the pelA and pslBCD deletions, respectively. Untagged mutants were created by Flp-mediated excision of the FRT-Gm-FRT cassette (where FRT is the Flp recombination target and Gm is a gentamicin resistance gene) by introducing pFlp2 into the mutants as described previously (25). Untagged mutants were cured for pFlp2 and verified by colony PCR using the aforementioned primer pairs. For the wspF deletion, the deletion vector pΔwspF was introduced into P. aeruginosa by biparental mating and single-crossover conjugants were selected by growth on ABTC agar supplemented with gentamicin. Double-crossover events were promoted by planktonic growth in LB medium without antibiotic selection, and the corresponding mutants were screened for by means of their wrinkly colony morphology. The correct deletion was verified by colony PCR using the primer pair wspF_fwd and wspF_rev.

Construction of ΔfleQ strain.

The pEX18Gm::ΔfleQ deletion vector was constructed in the following way. Overlap extension PCR using the primer pairs fleQ-1s/fleQ-1a and fleQ-2s/fleQ-2a was used to amplify a DNA fragment with a 1,482-bp in-frame deletion of the fleQ coding sequence. The fragment was inserted in the allelic exchange vector pEX18Gm (25). pEX18Gm::ΔfleQ was introduced in P. aeruginosa by E. coli S17-1 λpir-mediated biparental mating. The deletion was created using a standard method for two-step allelic exchange as described by Schweizer and Hoang (44) and was confirmed by PCR using the primers fleQ-os and fleQ-as flanking the deletion fragment.

Construction of PBAD::tpbB CTX chromosomal insertion.

The integration plasmid pDONRminiCTX2::PBADPA1120 was engineered for the conditional expression of the DGC TpbB (PA1120) and inserted into the chromosome to construct the P. aeruginosa strain PBADPA1120. PCR was used to amplify from pJN1120 (23) a 3.1-kb fragment comprising the araC-PBAD arabinose-inducible expression cassette (39) fused to tpbB. The PCR primer pair used, BBctxPBAD::1120attB1 and BBctxPBAD::1120attB2, contains attb1 and attb2 sites that allow recombination into the pDONRminiCTX2 integration plasmid (Joe Harrison, unpublished) using BP Clonase (Invitrogen), as suggested by the manufacturer. The resulting plasmid was introduced into P. aeruginosa by electroporation (10), where it integrates into the attB locus and the mini-CTX plasmid backbone is excised upon expression of Flp recombinase via pFLP2, as described by Hoang et al. (26).

Construction of c-di-GMP reporter strains.

The plasmid-based reporters pCdrA::gfpC and pCdrA::gfp(ASV)C were introduced into the P. aeruginosa ΔpelΔpsl and ΔpelΔpslΔwspF background strains by means of biparental mating. pCdrA::gfpS and pCdrA::gfp(ASV)S were introduced into the background strains by electroporation (10). The background strains were tagged with the mini-Tn7 reporter constructs from pTn7CdrA::gfpC and pTn7CdrA::gfp(ASV)C by means of four-parental mating with E. coli DH5α harboring the delivery vectors as donor strains and with E. coli strains harboring pUX-BF13 and pRK600 as helper strains.

Colony morphology and fluorescence intensity analysis.

The colony morphology and fluorescence intensity of the Copenhagen reporter strains were analyzed by streaking the strains on minimal medium plates and growing them for 20 h. The colonies were visualized using a Zeiss LSM710 confocal microscope equipped with a ×10 objective, a UV lamp, GFP filter sets, and a monochrome camera. Morphologies were visualized by bright-field microscopy, and fluorescence was visualized by epifluorescence microscopy. Pictures were taken using AxioVision software and combined using a standard graphics program.

Shake flask-based c-di-GMP reporter assay.

The Copenhagen reporter strains were assayed by growth in shake flasks in the following way. Strains were inoculated from fresh streaks on ABTC agar with gentamicin into a 50-ml shake flask with 15 ml ABTG+casA supplemented with gentamicin. After overnight (ON) growth at 185 rpm, the strains were diluted to an optical density at 600 nm (OD600) of 0.03 into 100 ml ABTG+casA supplemented with gentamicin in a 250-ml shake flask and grown for an additional 24 h at 185 rpm, with samples for OD600 and fluorescence measurements being withdrawn at regular intervals. Fluorescence was measured as arbitrary fluorescence intensity units (FIU) on a Turner Quantech digital filter fluorometer (Thermo Scientific) using a 490-nm narrow-band excitation filter, a 515-nm sharp-cut emission filter, and the raw fluorescence mode with gain code 11. For the sodium nitroprusside (SNP; Sigma) experiment, 250 μM, 31.25 μM, 2 μM, and 0.25 μM final concentrations were made from a stock solution of 50 mM SNP dissolved in Milli-Q water. Shake flasks containing SNP were incubated in the dark due to the light-sensitive nature of SNP.

Microtiter plate-based c-di-GMP reporter assay.

Microtiter plate-based assays with the Copenhagen reporter strains were carried out as follows: ON cultures of the strains were prepared as described above for the shake flask experiments (see above) and diluted to an OD600 of 0.03 in 100-ml shake flasks with 30 ml ABTG+casA supplemented with gentamicin. Growth was measured manually until the OD600 reached 0.5, at which point 300 μl of the cultures was added to the wells of a black-welled 96-well microtiter plate (Nunc) and incubated in a Victor2 (Perkin Elmer) plate reader heated to 37°C and set up to measure OD450 and green fluorescence (arbitrary GFP units) every 30 min for approximately 22 h. The plates were shaken in an orbital pattern (3-mm diameter) at normal speed for 10 min before and after each round of measurements to optimize growth. For the SNP experiment, 2-fold serial dilutions starting from 250 μM SNP were made from a 50 mM stock of SNP dissolved in Milli-Q water. To maintain the OD600 at 0.5 for the pregrown reporter strains, the cell culture was used to make the serial dilutions.

Analysis of fleQ regulation and PA1120 induction in Seattle reporter strains.

The activity of the Seattle reporter strains was assayed in the following way. Strains were inoculated from fresh streaks on LB agar supplemented with gentamicin into 16-mm test tubes with 3 ml LB broth supplemented with gentamicin. After growth overnight at 250 rpm, the strains were diluted in triplicate (100 μl into 3 ml LB medium supplemented with gentamicin in a 16-mm test tube) and grown to mid-logarithmic growth phase (approximately 2.5 h). Arabinose was also supplemented when indicated at a final concentration of 0.2% (wt/vol) in studies where the conditional expression of the DGC TpbB was evaluated. Samples were concentrated 2 times by centrifugation, and the supernatant was removed. Bacterial pellets were suspended in phosphate-buffered saline and aliquoted into a Costar 96-well black clear-bottom microtiter plate (Corning) and measured for fluorescence (excitation = 485 nm, emission = 535 nm) and optical density (595 nm) using a Tecan GENios plate reader. Data are presented as relative fluorescent units (RFU), which are arbitrary fluorescence intensity units corrected for cell density.

Nucleotide extraction and quantitative c-di-GMP measurements.

Nucleotides were extracted as previously described (13). Briefly, 990 μl from a culture grown to mid- to late exponential phase was spiked with 10 μl of 10 mM 2-chloro-AMP (Biolog) as internal standard and immediately treated with 70% perchloric acid (Sigma) to a final concentration of 0.6 M. The pHs of the soluble fractions containing nucleotides were adjusted with KHCO3 as previously described (23), prior to liquid chromatography-tandem mass spectrometry (LC-MS/MS) measurements of the c-di-GMP levels. The protein-containing precipitates were quantified by the Bradford assay (Bio-Rad) and used to normalize c-di-GMP measurements.


Construction of c-di-GMP-responsive reporters.

For construction of the c-di-GMP reporters, we first set out to identify a suitable gene that was highly responsive to fluctuations in the intracellular level of c-di-GMP in P. aeruginosa. One gene, cdrA (PA4625), encoding a large adhesin (9) was found to be highly upregulated in response to increased levels of c-di-GMP (9, 24). We expected the cdrA promoter to be a good candidate as part of a transcriptional fusion with gfp that could act as a reporter of c-di-GMP levels in P. aeruginosa.

The exact location of the cdrA promoter, including the −35, −10, and other regulatory sequences, is unknown, so for the Copenhagen reporters, we arbitrarily chose to amplify the region of the genome from 23 to 221 bp upstream of the start codon. The gap between the amplified sequence and the start codon of cdrA was used to omit the native ribosomal binding site (RBS) in the reporter constructs. Instead, we used an artificial RBS to enhance translation from the gfp mRNA in order to increase the signal related to c-di-GMP-responsive transcription from the promoter.

We created cassettes (Fig. 1A) consisting of the cdrA promoter fused to the artificial RBS and gfp. Because the kinetics of c-di-GMP-induced transcription from the cdrA promoter were unknown, we chose to construct fusions encoding either the stable GFP (Mut3) protein or the unstable GFP (ASV) protein (2). In these constructs, gfp is situated at an optimal distance from the RBS to further enhance translation (2). In addition, two transcriptional terminators, interspersed by a chloramphenicol resistance gene, are located downstream of gfp to efficiently terminate transcription, minimizing unnecessary read-through from RNA polymerase.

Fig 1
Schematic drawing of the Copenhagen (A) and Seattle (B) c-di-GMP reporter cassettes. (A) The cassette consists of a transcriptional fusion between the promoter from cdrA (PcdrA) and a gene encoding either stable GFP or unstable GFP (both designated gfp ...

pUCP22Not and pBK-miniTn7-ΩGm were used as final destination vectors for the reporter cassettes to create plasmid-based and chromosome-integrated reporters, respectively. pUCP22Not contains a lac promoter directly upstream of the multiple-cloning site (MCS), and as P. aeruginosa does not contain lacI, the promoter allows read-through and expression of gfp even in the absence of c-di-GMP, leading to a false signal. Therefore, the pUCP22-Not-based reporters pCdrA::gfpC and pCdrA::gfp(ASV)C were constructed such that the inserted cassettes had the coding sequence of gfp situated on the complementary strand with regard to the direction of the lac promoter. pBK-miniTn7-ΩGm is a pUC-based vector that does not replicate in P. aeruginosa. It carries a mini-Tn7 transposon without the transposase genes and allows stable chromosomal tagging at a neutral locus in the genome of P. aeruginosa when transposase genes are provided transiently in trans.

Two genetic backgrounds were chosen for the reporter constructs, a wild-type P. aeruginosa PAO1 strain and an isogenic wspF deletion mutant. Deletion of wspF results in elevated levels of c-di-GMP in P. aeruginosa through the continuous activation of the DGC WspR, a component of the Wsp signal transduction system (24). A ΔwspF strain containing the c-di-GMP reporter is predicted to have an increased level of fluorescence compared to the wild-type strain and could be used as the target strain for inhibitor screening. Additionally, we deleted the genes pelA and pslBCD in both the wild-type and wspF mutant, resulting in an inability to produce Pel and Psl polysaccharides. Pel and Psl are important parts of the P. aeruginosa extracellular matrix during biofilm growth (16), and their production is regulated positively by c-di-GMP (24, 34, 45), which results in bacterial aggregation in planktonic culture when c-di-GMP levels are elevated. Aggregation complicates the OD measurements used to monitor growth of bacteria, which is important during identification of inhibitors that are nontoxic to the cells. Therefore, we chose to work with reporters in the nonaggregating Δpel Δpsl strains. Based on LC-MS/MS measurements, the cellular c-di-GMP content was estimated to be 10.9 (standard deviation [SD], 4.2) and 77.0 (SD, 6.5) pmol c-di-GMP/mg total protein in mid- to late-log-phase cells of strains ΔpslΔpel and ΔwspFΔpslΔpel, respectively. The wspF deletion thus resulted in a 7-fold increase in the cellular level of c-di-GMP.

The Seattle series of c-di-GMP reporters (Fig. 1B) was created in a fashion similar to that for the Copenhagen reporters. The reporters were based on the plasmids pMH487 and pMH489 harboring promoterless genes encoding stable and unstable variants of gfp, respectively. Both plasmids harbor an RNase III splice site directly upstream of gfp. To regulate the expression of the gfp variants, the cdrA promoter and part of the coding sequence were inserted in front of the GFP genes, thereby creating pCdrA::gfpS and pCdrA::gfp(ASV)S.

The c-di-GMP reporters respond to the cellular levels of c-di-GMP.

The ability of the c-di-GMP reporters to fluoresce in accordance with c-di-GMP levels was visualized by epifluorescence microscopy of 1-day-old colonies on minimal medium. Comparing the plasmid-based to the chromosome-integrated reporters, it became clear that the latter were not suited for the intended screening purposes due to a low level of fluorescence (data not shown). We decided to use plasmid-based reporters for the further development of screening assays. The wspF mutant harboring elevated levels of c-di-GMP displayed the brightest colonies, indicating that the fluorescence intensity of the reporters is indeed correlated with the intracellular level of c-di-GMP, as hypothesized (Fig. 2). In addition, the fluorescence intensity pictures showed that the reporters with unstable GFP fluoresced less than the reporters with stable GFP, confirming the temporal instability of GFP (ASV) (Fig. 2).

Fig 2
Colony morphology (top) and fluorescence intensity (bottom) of the plasmid-based reporter strains. (A) P. aeruginosa PAO1 ΔpelΔpsl/pCdrA::gfpC (normal c-di-GMP level, stable GFP); (B) ΔwspFΔpelΔpsl/pCdrA::gfpC (increased ...

A previous study by Hickman and Harwood (23) indicated that transcription of the cdrA gene is repressed by the transcriptional regulator FleQ in P. aeruginosa and that c-di-GMP can bind to the FleQ regulator and cause derepression, releasing FleQ from the promoter. The reporters were placed in a ΔfleQ strain and in a ΔwspF strain to investigate if this regulatory pattern could be observed for our reporters as well. We found that the ΔfleQ strain with the reporter displayed a significantly higher level of fluorescence than the wild-type with the reporter, indicating that the regulation of the reporter constructs works as anticipated (Fig. 3). The level of fluorescence of the ΔwspF strain with the reporter was comparable to that seen for the ΔfleQ strain with the reporter, indicating that the level of c-di-GMP present in the ΔwspF strain results in comparable derepression of the FleQ-regulated cdrA promoter activity.

Fig 3
Fluorescence from P. aeruginosa PAO1/pCdrA::gfp(ASV)S, ΔfleQ/pCdrA::gfp(ASV)S, ΔwspFΔpelΔpsl/pCdrA::gfp(ASV)S, and vector controls (VC). RFU values are arbitrary fluorescence intensity units corrected for cell density. ...

Development of screening assays.

To determine the kinetics of gfp transcription from the cdrA promoter, the reporters were grown in shake flasks and monitored for growth and fluorescence. Figure 4A shows that transcription from the cdrA promoter is related to the high levels of c-di-GMP induced during the early stationary growth phase and then kept at a constant high level over time.

Fig 4
Test of the plasmid-based reporter strains in shake flasks (A) and microtiter plates (B). (Left) Growth measurements; (right) fluorescence measurements. Results are representative of three independent experiments. ■, P. aeruginosa PAO1 Δ ...

To efficiently screen for compounds affecting the c-di-GMP level in P. aeruginosa, we developed a microtiter plate-based setup which allows screening of several compounds simultaneously. We grew dilutions of outgrown cultures in shake flasks until they reached the mid-logarithmic growth phase, after which they were transferred undiluted to a microtiter plate and incubated in a plate reader. As shown in Fig. 4B, the fluorescent kinetics resembled those seen with the shake flask setup, making the assay suitable for screening purposes.

As seen in Fig. 4, the unstable GFP (ASV) resulted in a lower ratio between strain ΔwspFΔpelΔpsl and strain ΔpelΔpsl than was the case with the strains containing the stable GFP (Mut3). Consequently, to maximize the signal-to-noise level, the strains containing the stable GFP would be preferred for screening purposes. It is also evident from Fig. 4 that the high level of fluorescence obtained with the strain ΔwspFΔpelΔpsl background will be better suited for screening purposes than the low level of fluorescence obtained with the strain ΔpelΔpsl background. The strain P. aeruginosa ΔwspFΔpelΔpsl/pCdrA::gfp would therefore be preferred for screening in our setup.

Proof of concept.

We subsequently wanted to establish proof of concept that the reporter strain can be used to monitor drug-induced changes in the intracellular level of c-di-GMP. To this end, we treated the P. aeruginosa ΔwspFΔpelΔpsl/pCdrA::gfpC reporter with the compound sodium nitroprusside (SNP). SNP is a nitrogen monoxide (NO)-releasing compound that has been shown to induce dispersal of established P. aeruginosa biofilms, evidently by NO induction of a phosphodiesterase, thereby decreasing the intracellular levels of c-di-GMP (5, 6). Initially, the reporter strain was treated with 2-fold serial dilutions of SNP in the microtiter plate assay (Fig. 5A). The treatment showed that over a range of concentrations the compound decreased the fluorescent levels of the reporter without affecting growth, indicating that cdrA::gfp transcription was reduced as a result of decreased c-di-GMP levels within the bacteria. For a subset of concentrations, the results were verified with the more sensitive shake-flask setup (Fig. 5B). There was a direct correlation between the SNP concentration and decrease in fluorescence for all concentrations except the treatment with 250 μM SNP. At this high concentration, the level of NO released presumably could impose stresses on the bacteria, resulting in changes in the c-di-GMP metabolism, other than what can be attributed to PDE activation. These results indicate that the reporter can be used to monitor drug-induced changes in c-di-GMP levels.

Fig 5
Treatment of P. aeruginosa PAO1 ΔwspFΔpelΔpsl/pCdrA::gfpC with SNP in microtiter plates (A) and shake flasks (B). (Left) Growth measurements; (right) fluorescence measurements. Results are based on the Copenhagen group of reporters ...

Investigating inhibition of different DGCs.

The results described above are based on a wspF background strain displaying a high level of fluorescence from our reporters due to the increased level of c-di-GMP stemming from WspR deregulation. However, P. aeruginosa contains several active DGCs that can all, presumably, affect cellular levels of c-di-GMP. It was important to determine if the reporters would respond to increased c-di-GMP levels originating from other DGCs, in addition to WspF, making it possible to test inhibitor candidates against multiple DGCs. To this end, the active DGC TpbB (33, 47) was cloned under the control of the arabinose-inducible promoter AraC-PBAD, allowing conditional expression upon arabinose induction, and integrated into the chromosome for these studies. As shown in Fig. 6, overexpression of tpbB results in increased fluorescence from the c-di-GMP reporter at levels comparable to those for the ΔwspF strain. This result indicates that the reporters can be used to monitor effects on c-di-GMP levels based on the activity of additional DGCs other than WspR.

Fig 6
Fluorescence from P. aeruginosa PAO1/pCdrA::gfp(ASV)S, ΔwspFΔpelΔpsl/pCdrA::gfp(ASV)S, ΔpelΔpsl PBAD::tpbB/pCdrA::gfp(ASV)S, and vector controls (VC). RFU values are arbitrary fluorescence intensity units corrected ...


In the present paper, we have described the development of two similar series of fluorescent reporters that can form the basis for genetic and chemical biology approaches to alteration of the level of c-di-GMP in P. aeruginosa and potentially other bacteria as well. The reporters are based on transcriptional fusions between the c-di-GMP-responsive cdrA promoter and gfp. The cdrA promoter was chosen because transcriptome analyses indicate that the level of cdrA transcription is regulated by the level of c-di-GMP in the bacteria (9, 24). Without prior knowledge of the exact location of the regulatory elements within the cdrA promoter region, the Copenhagen group of reporters was constructed by amplifying 200 bp upstream of the start codon while at the same time omitting the sequence likely containing the native RBS. With a fusion of the amplified promoter region to gfp containing an optimized RBS, we were able to see a clear difference in the fluorescence level in the ΔwspF compared to the wspF wild-type background strain of P. aeruginosa. This difference is attributed to their known difference in internal c-di-GMP levels (24), and it was corroborated by LC-MS/MS analyses of the c-di-GMP content in the ΔpelΔpsl and ΔwspFΔpelΔpsl background strains used in this study.

The Seattle group of reporters was created by amplifying a larger part of the cdrA promoter, including the native RBS and a small part of the coding sequence, and fusing it to promoterless GFP vectors. These reporters responded positively to an increased level of c-di-GMP in the same manner as the Copenhagen reporters, yielding a clear indication that the binding site for the c-di-GMP-responsive regulatory element had been included in both groups of constructs and that they function as expected. The regulatory element was shown to be the transcriptional regulator FleQ, as a fleQ mutant harboring a c-di-GMP reporter showed a high fluorescent output similar to that of a wspF mutant harboring the c-di-GMP reporter. This result is consistent with previous observations linking c-di-GMP to increased cdrA transcription via sequestration of FleQ (23). We anticipate that the c-di-GMP level reporters may work in other bacterial species that produce FleQ homologs. It is also likely that the reporters will work in other bacterial species if they are modified so that the P. aeruginosa fleQ gene is included in the reporter construct.

Traditionally, measurements of c-di-GMP levels have been made directly on the molecule using thin-layer chromatography or mass spectrometry on cellular extracts. These labor-intensive methods have the advantage of measuring the amount of c-di-GMP directly but are unsuitable for screening purposes. In addition, fluorescence-based measurements of c-di-GMP levels have been described recently. One study utilizes the discovery that thiazole orange fluoresces upon formation of a specific complex with c-di-GMP (38). The method requires lysis of the bacteria but is less laborious than the standard methods. However, it is sensitive to the presence of nucleic acids which bind thiazole orange and gives rise to fluorescence. Another method employs a genetically engineered c-di-GMP binding protein fused to two fluorescent proteins at the N and C termini (11). Binding of c-di-GMP induces a conformational change that decreases the amount of fluorescence observed due to fluorescence resonance energy transfer (FRET) between the fluorescent proteins. The method itself is ingenious, but the small amount of fluorescence usually obtained via FRET might be less than that required for sufficient sensitivity during screening. In contrast to these methods, we have created a cell-based c-di-GMP-sensitive reporter system similar to the ones employed in the discovery of quorum-sensing inhibitors in P. aeruginosa. An analogous approach has also recently been described in E. coli (3). The approach relies on increased binding of Congo red to cellulose produced by cells in response to elevated levels of c-di-GMP resulting from overexpression of the DGC AdrA. Compared to the present setup, the visual inspection of Congo red binding gives the assay a limited dynamic range less suitable for high-throughput screening where subtle differences in c-di-GMP levels are also of relevance.

The reporters in this study were constructed using both stable and unstable GFP and were made plasmid based or transposon integrated. From the epifluorescence microscope observations, it became clear that the plasmid-based reporters, as expected, showed the highest level of fluorescence and were best suited for screening purposes. In addition, testing of the plasmid-based reporter strains showed that the use of stable GFP gave adequate fluorescence levels, making the plasmid-based reporter with stable GFP the reporter of choice in the screening for compounds affecting c-di-GMP metabolism. The other reporter strains could still be employed in later steps of the process. The unstable GFP could be used to monitor the change in c-di-GMP levels during longer periods of growth in flow-cell setups investigating biofilm formation over time. Experiments using these reporters should provide information regarding spatiotemporal expression of cdrA in P. aeruginosa biofilms and would be valuable in describing the antipathogenic effects of specific compounds that decrease fluorescence from the reporter in the initial screen.

The deletion of wspF used to increase the level of c-di-GMP causes increased polysaccharide production and therefore intense clumping of cells grown in liquid culture, making growth monitoring by means of optical density impossible. For correct measurements of growth, the background strains used here carried mutations abolishing polysaccharide production. However, the inability to produce Pel and Psl polysaccharides results in a fluorescent output from the reporters lower than what is seen with polysaccharide-producing strains harboring the reporters (data not shown). This is in accordance with previously published reverse transcription-PCR data on cdrA expression showing the same trend (9). It thus appears that the presence of polysaccharides somehow affects c-di-GMP metabolism in P. aeruginosa.

Besides being able to distinguish the two background strains with different levels of c-di-GMP on the basis of their fluorescent output, it was crucial that the reporter showed sufficient sensitivity to gauge intermediate c-di-GMP levels stemming from changes in the metabolism caused by c-di-GMP level-altering compounds. We tested this by treatment of the c-di-GMP-overproducing reporter strain with the NO-releasing compound SNP. SNP has previously been shown to reduce c-di-GMP levels 2-fold in P. aeruginosa at two different μM concentrations (6). In our study, we could observe different degrees of changes in the fluorescence output over a range of concentrations, indicating that the reporter was sensitive enough to distinguish small changes in c-di-GMP levels. Compared to the untreated reporter strain, the total decrease in fluorescence was roughly 2- to 3-fold for the lower concentrations of SNP tested, which is comparable to previous observations for the cellular c-di-GMP levels (6).

P. aeruginosa contains 33 GGDEF domain proteins (including domains with degenerate motifs) (33), of which one-fourth have been found, at present, to be active DGCs (24, 33, 35, 36). This has raised the question whether the intracellular pool of c-di-GMP is compartmentalized or global and how the phenotypes related to c-di-GMP signaling are regulated. Recent research shows that the two DGCs RoeA and SadC regulate different aspects of biofilm formation (37), indicating that c-di-GMP might be sequestered as local pools that are regulated by distinct DGCs and PDEs. This suggests that potent antipathogenic drugs targeting c-di-GMP production should be able to inhibit several DGCs. This could complicate our choice of working with a reporter background where WspR is the dominating DGC, due to the wspF deletion, contributing to the increased level of c-di-GMP. The use of this reporter background to discover DGC inhibitors will likely result in hits that mainly affect WspR. We showed, however, that overexpression of another DGC, TpbB, caused a similar increase in the fluorescent readout from the reporters, indicating that such constructs could favorably be used to test initial drug candidates against several DGCs, determining if they display a broad activity increasing the desired antipathogenic effect.

A comparative analysis of the residues comprising the active site of the different P. aeruginosa DGCs shows a high degree of similarity indicating that they share the same conformation and thus should be able to bind the same inhibitor (unpublished analysis). We therefore believe that it will be possible to identify compounds that inhibit several DGCs in P. aeruginosa and other bacteria and thus will be suitable leads in the development of potent antipathogenic compounds. In our future work, we will use the constructed reporters in screens for antipathogenic drugs and to obtain knowledge on basic P. aeruginosa biofilm biology.


We thank Bettina Andreasen for help with construction of the Copenhagen group of reporters. Joe J. Harrison is gratefully acknowledged for providing the pDONRminiCTX2 plasmid.

This work was supported by grants from the Danish Strategic Research Council and the Danish Council for Independent Research and by a grant from the Novo Nordisk Foundation. B.R.B. was supported by a Cystic Fibrosis Foundation Research Development Program postdoctoral fellowship.


Published ahead of print 11 May 2012


1. Alhede M, et al. 2009. Pseudomonas aeruginosa recognizes and responds aggressively to the presence of polymorphonuclear leukocytes. Microbiology 155:3500–3508 [PubMed]
2. Andersen JB, et al. 1998. New unstable variants of green fluorescent protein for studies of transient gene expression in bacteria. Appl. Environ. Microbiol. 64:2240–2246 [PMC free article] [PubMed]
3. Antoniani D, Bocci P, Maciag A, Raffaelli N, Landini P. 2010. Monitoring of diguanylate cyclase activity and of cyclic-di-GMP biosynthesis by whole-cell assays suitable for high-throughput screening of biofilm inhibitors. Appl. Microbiol. Biotechnol. 85:1095–1104 [PubMed]
4. Bao Y, Lies DP, Fu H, Roberts GP. 1991. An improved Tn7-based system for the single-copy insertion of cloned genes into chromosomes of gram-negative bacteria. Gene 109:167–168 [PubMed]
5. Barraud N, et al. 2006. Involvement of nitric oxide in biofilm dispersal of Pseudomonas aeruginosa. J. Bacteriol. 188:7344–7353 [PMC free article] [PubMed]
6. Barraud N, et al. 2009. Nitric oxide signaling in Pseudomonas aeruginosa biofilms mediates phosphodiesterase activity, decreased cyclic di-GMP levels, and enhanced dispersal. J. Bacteriol. 191:7333–7342 [PMC free article] [PubMed]
7. Bjarnsholt T, et al. 2005. Pseudomonas aeruginosa tolerance to tobramycin, hydrogen peroxide and polymorphonuclear leukocytes is quorum-sensing dependent. Microbiology 151:373–383 [PubMed]
8. Bjarnsholt T, Tolker-Nielsen T, Hoiby N, Givskov M. 2010. Interference of Pseudomonas aeruginosa signalling and biofilm formation for infection control. Expert Rev. Mol. Med. 12:e11. [PubMed]
9. Borlee BR, et al. 2010. Pseudomonas aeruginosa uses a cyclic-di-GMP-regulated adhesin to reinforce the biofilm extracellular matrix. Mol. Microbiol. 75:827–842 [PMC free article] [PubMed]
10. Choi KH, Kumar A, Schweizer HP. 2006. A 10-min method for preparation of highly electrocompetent Pseudomonas aeruginosa cells: application for DNA fragment transfer between chromosomes and plasmid transformation. J. Microbiol. Methods 64:391–397 [PubMed]
11. Christen M, et al. 2010. Asymmetrical distribution of the second messenger c-di-GMP upon bacterial cell division. Science 328:1295–1297 [PMC free article] [PubMed]
12. Clark DJ, Maaløe O. 1967. DNA replication and the division cycle in Escherichia coli. J. Mol. Biol. 23:99–112
13. Colvin KM, et al. 19 December 2011. The Pel and Psl polysaccharides provide Pseudomonas aeruginosa structural redundancy within the biofilm matrix. Environ. Microbiol. doi:10.1111/j.1462-2920.2011.02657.x [PMC free article] [PubMed]
14. Costerton JW, Stewart PS, Greenberg EP. 1999. Bacterial biofilms: a common cause of persistent infections. Science 284:1318–1322 [PubMed]
15. Fazli M, et al. 2011. The CRP/FNR family protein Bcam1349 is a c-di-GMP effector that regulates biofilm formation in the respiratory pathogen Burkholderia cenocepacia. Mol. Microbiol. 82:327–341 [PubMed]
16. Friedman L, Kolter R. 2004. Two genetic loci produce distinct carbohydrate-rich structural components of the Pseudomonas aeruginosa biofilm matrix. J. Bacteriol. 186:4457–4465 [PMC free article] [PubMed]
17. Gjermansen M, Nilsson M, Yang L, Tolker-Nielsen T. 2010. Characterization of starvation-induced dispersion in Pseudomonas putida biofilms: genetic elements and molecular mechanisms. Mol. Microbiol. 75:815–826 [PubMed]
18. Gjermansen M, Ragas P, Tolker-Nielsen T. 2006. Proteins with GGDEF and EAL domains regulate Pseudomonas putida biofilm formation and dispersal. FEMS Microbiol. Lett. 265:215–224 [PubMed]
19. Hentzer M, Givskov M. 2003. Pharmacological inhibition of quorum sensing for the treatment of chronic bacterial infections. J. Clin. Invest. 112:1300–1307 [PMC free article] [PubMed]
20. Hentzer M, et al. 2002. Inhibition of quorum sensing in Pseudomonas aeruginosa biofilm bacteria by a halogenated furanone compound. Microbiology 148:87–102 [PubMed]
21. Hentzer M, et al. 2003. Attenuation of Pseudomonas aeruginosa virulence by quorum sensing inhibitors. EMBO J. 22:3803–3815 [PubMed]
22. Herrero M, de Lorenzo V, Timmis KN. 1990. Transposon vectors containing non-antibiotic resistance selection markers for cloning and stable chromosomal insertion of foreign genes in gram-negative bacteria. J. Bacteriol. 172:6557–6567 [PMC free article] [PubMed]
23. Hickman JW, Harwood CS. 2008. Identification of FleQ from Pseudomonas aeruginosa as a c-di-GMP-responsive transcription factor. Mol. Microbiol. 69:376–389 [PMC free article] [PubMed]
24. Hickman JW, Tifrea DF, Harwood CS. 2005. A chemosensory system that regulates biofilm formation through modulation of cyclic diguanylate levels. Proc. Natl. Acad. Sci. U. S. A. 102:14422–14427 [PubMed]
25. Hoang TT, Karkhoff-Schweizer RR, Kutchma AJ, Schweizer HP. 1998. A broad-host-range Flp-FRT recombination system for site-specific excision of chromosomally-located DNA sequences: application for isolation of unmarked Pseudomonas aeruginosa mutants. Gene 212:77–86 [PubMed]
26. Hoang TT, Kutchma AJ, Becher A, Schweizer HP. 2000. Integration-proficient plasmids for Pseudomonas aeruginosa: site-specific integration and use for engineering of reporter and expression strains. Plasmid 43:59–72 [PubMed]
27. Hoiby N, Ciofu O, Bjarnsholt T. 2010. Pseudomonas aeruginosa biofilms in cystic fibrosis. Future Microbiol. 5:1663–1674 [PubMed]
28. Jensen PO, et al. 2007. Rapid necrotic killing of polymorphonuclear leukocytes is caused by quorum-sensing-controlled production of rhamnolipid by Pseudomonas aeruginosa. Microbiology 153:1329–1338 [PubMed]
29. Kazmierczak BI, Lebron MB, Murray TS. 2006. Analysis of FimX, a phosphodiesterase that governs twitching motility in Pseudomonas aeruginosa. Mol. Microbiol. 60:1026–1043 [PMC free article] [PubMed]
30. Kessler B, de Lorenzo V, Timmis KN. 1992. A general system to integrate lacZ fusions into the chromosomes of gram-negative eubacteria: regulation of the Pm promoter of the TOL plasmid studied with all controlling elements in monocopy. Mol. Gen. Genet. 233:293–301 [PubMed]
31. Kirisits MJ, Prost L, Starkey M, Parsek MR. 2005. Characterization of colony morphology variants isolated from Pseudomonas aeruginosa biofilms. Appl. Environ. Microbiol. 71:4809–4821 [PMC free article] [PubMed]
32. Koch B, Jensen LE, Nybroe O. 2001. A panel of Tn7-based vectors for insertion of the gfp marker gene or for delivery of cloned DNA into Gram-negative bacteria at a neutral chromosomal site. J. Microbiol. Methods 45:187–195 [PubMed]
33. Kulasakara H, et al. 2006. Analysis of Pseudomonas aeruginosa diguanylate cyclases and phosphodiesterases reveals a role for bis-(3′-5′)-cyclic-GMP in virulence. Proc. Natl. Acad. Sci. U. S. A. 103:2839–2844 [PubMed]
34. Lee VT, et al. 2007. A cyclic-di-GMP receptor required for bacterial exopolysaccharide production. Mol. Microbiol. 65:1474–1484 [PMC free article] [PubMed]
35. Malone JG, et al. 2010. YfiBNR mediates cyclic di-GMP dependent small colony variant formation and persistence in Pseudomonas aeruginosa. PLoS Pathog. 6:e1000804 doi:10.1371/journal.ppat.1000804 [PMC free article] [PubMed]
36. Merritt JH, Brothers KM, Kuchma SL, O'Toole GA. 2007. SadC reciprocally influences biofilm formation and swarming motility via modulation of exopolysaccharide production and flagellar function. J. Bacteriol. 189:8154–8164 [PMC free article] [PubMed]
37. Merritt JH, et al. 2010. Specific control of Pseudomonas aeruginosa surface-associated behaviors by two c-di-GMP diguanylate cyclases. mBio 1:e00183–10 doi:10.1128/mBio.00183-10 [PMC free article] [PubMed]
38. Nakayama S, et al. 2011. Thiazole orange-induced c-di-GMP quadruplex formation facilitates a simple fluorescent detection of this ubiquitous biofilm regulating molecule. J. Am. Chem. Soc. 133:4856–4864 [PubMed]
39. Newman JR, Fuqua C. 1999. Broad-host-range expression vectors that carry the l-arabinose-inducible Escherichia coli araBAD promoter and the araC regulator. Gene 227:197–203 [PubMed]
40. Rasmussen TB, et al. 2005. Identity and effects of quorum-sensing inhibitors produced by Penicillium species. Microbiology 151:1325–1340 [PubMed]
41. Ryan RP, et al. 2006. Cell-cell signaling in Xanthomonas campestris involves an HD-GYP domain protein that functions in cyclic di-GMP turnover. Proc. Natl. Acad. Sci. U. S. A. 103:6712–6717 [PubMed]
42. Ryjenkov DA, Tarutina M, Moskvin OV, Gomelsky M. 2005. Cyclic diguanylate is a ubiquitous signaling molecule in bacteria: insights into biochemistry of the GGDEF protein domain. J. Bacteriol. 187:1792–1798 [PMC free article] [PubMed]
43. Schmidt AJ, Ryjenkov DA, Gomelsky M. 2005. The ubiquitous protein domain EAL is a cyclic diguanylate-specific phosphodiesterase: enzymatically active and inactive EAL domains. J. Bacteriol. 187:4774–4781 [PMC free article] [PubMed]
44. Schweizer HP, Hoang TT. 1995. An improved system for gene replacement and xylE fusion analysis in Pseudomonas aeruginosa. Gene 158:15–22 [PubMed]
45. Starkey M, et al. 2009. Pseudomonas aeruginosa rugose small-colony variants have adaptations that likely promote persistence in the cystic fibrosis lung. J. Bacteriol. 191:3492–3503 [PMC free article] [PubMed]
46. Stover CK, et al. 2000. Complete genome sequence of Pseudomonas aeruginosa PAO1, an opportunistic pathogen. Nature 406:959–964 [PubMed]
47. Ueda A, Wood TK. 2010. Tyrosine phosphatase TpbA of Pseudomonas aeruginosa controls extracellular DNA via cyclic diguanylic acid concentrations. Environ. Microbiol. 2:449–455 [PMC free article] [PubMed]
48. West SE, Schweizer HP, Dall C, Sample AK, Runyen-Janecky LJ. 1994. Construction of improved Escherichia-Pseudomonas shuttle vectors derived from pUC18/19 and sequence of the region required for their replication in Pseudomonas aeruginosa. Gene 148:81–86 [PubMed]

Articles from Applied and Environmental Microbiology are provided here courtesy of American Society for Microbiology (ASM)