About the Authors:
Tsiry Rasamiravaka
Contributed equally to this work with: Tsiry Rasamiravaka, Olivier M. Vandeputte
Affiliations Laboratoire de Biotechnologie Végétale, Université Libre de Bruxelles, Gosselies, Belgium, Laboratoire de Formation et de Recherche en Biologie Médicale, Faculté de Médecine, Université d'Antananarivo, Antananarivo, Madagascar
Olivier M. Vandeputte
Contributed equally to this work with: Tsiry Rasamiravaka, Olivier M. Vandeputte
Current address: Laboratoire de Biotechnologie Végétale, Université Libre de Bruxelles (ULB), Gosselies, Belgium.
Affiliation: Laboratoire de Biotechnologie Végétale, Université Libre de Bruxelles, Gosselies, Belgium
Laurent Pottier
Affiliation: Laboratoire de Pharmacognosie, de Bromatologie et de Nutrition Humaine, Université Libre de Bruxelles, Brussels, Belgium
Joelle Huet
Affiliation: Laboratoire de Pharmacognosie, de Bromatologie et de Nutrition Humaine, Université Libre de Bruxelles, Brussels, Belgium
Christian Rabemanantsoa
Affiliation: Laboratoire de Biodiversité et de Biotechnologie, Institut Malgache de Recherches Appliquées, Antananarivo, Madagascar
Martin Kiendrebeogo
Affiliations Laboratoire de Biotechnologie Végétale, Université Libre de Bruxelles, Gosselies, Belgium, Laboratoire de Biochimie et de Chimie Appliquées, Université de Ouagadougou, Ouagadougou, Burkina Faso
Abel Andriantsimahavandy
Affiliation: Laboratoire de Formation et de Recherche en Biologie Médicale, Faculté de Médecine, Université d'Antananarivo, Antananarivo, Madagascar
Andry Rasamindrakotroka
Affiliation: Laboratoire de Formation et de Recherche en Biologie Médicale, Faculté de Médecine, Université d'Antananarivo, Antananarivo, Madagascar
Caroline Stévigny
Affiliation: Laboratoire de Pharmacognosie, de Bromatologie et de Nutrition Humaine, Université Libre de Bruxelles, Brussels, Belgium
Pierre Duez
Affiliations Laboratoire de Pharmacognosie, de Bromatologie et de Nutrition Humaine, Université Libre de Bruxelles, Brussels, Belgium, Service de Chimie Thérapeutique et de Pharmacognosie, Université de Mons, Mons, Belgium
Mondher El Jaziri
* E-mail: [email protected]
Affiliation: Laboratoire de Biotechnologie Végétale, Université Libre de Bruxelles, Gosselies, Belgium
Introduction
Over the last decades, pathogenic bacteria have presented an increasing multi-drug resistance prevalence all over the world [1, 2], a situation that has stimulated the search for new potential antibacterial drug targets [3, 4]. Inhibiting the bacterial virulence without killing the pathogen is an attractive anti-pathogenic approach that is increasingly explored [5, 6] with the putative advantage to generate less selective pressure as compared to antibiotics [7]. Quorum sensing (QS), a bacterial cell-to-cell communication, is used by many bacteria to detect their critical cell density by producing and perceiving diffusible signal molecules in order to coordinate a common behavior such as the expression and regulation of virulence factors, motility and biofilm formation [8, 9]. Therefore, the inhibition of QS systems might be a more valuable approach than targeting a single particular virulence factor for therapeutic or prophylactic control of infections.
The opportunistic pathogen P. aeruginosa is known to be an important human, animal and plant pathogen that produces several virulence factors. Its QS systems are probably the best-characterized among Gram-negative bacteria [10]. P. aeruginosa possesses two main QS systems (las and rhl) which drive the production (by the synthetases LasI and RhlI) and the detection (by the transcription factors LasR and RhlR) of the acylhomoserine lactones (AHL) N-(3-oxododecanoyl)-L-homoserine lactone (3-oxo-C12-HSL) and N-butanoyl-L-homoserine lactone (C4-HSL), respectively [11]. The las system controls LasB elastase, LasA protease, Apr alkaline protease, and exotoxin A [12] while the rhl system enhances the production of rhamnolipids, pyocyanin, LasB elastase, hydrogen cyanide, and cytotoxic lectins which are all involved in cellular toxicity and acute infection [13, 14]. The las and the rhl systems are organized in a hierarchical manner such that the las system regulates the rhl system at the transcriptional and post-transcriptional levels [15, 16]. In addition, P. aeruginosa releases a third intercellular signal, 2-heptyl-hydroxy-4-quinolone (designated the Pseudomonas quinolone signal [PQS]), which interacts with the acylhomoserine lactones (AHLs) systems in an intricate way [17]. The PQS system is incorporated into the QS hierarchy in times of cell stress, and acts as a link between the las and rhl quorum-sensing systems [18]. In this QS regulatory cascade, the las and rhl systems are positively influenced by the global activator GacA and the global regulator Vfr at both the transcriptional and post-transcriptional levels [19, 20].
Biofilms are surface-associated communities enclosed within an extracellular matrix [21] mainly composed of polysaccharides, proteins, nucleic acids, lipids and other macromolecules and chemicals [22]. Particularly, extracellular polysaccharides are a crucial component of the matrix, and carry out a range of functions such as promoting attachment to surfaces and other cells, building and maintaining biofilm structure, as well as protecting the cells against environmental assaults and predation, including antimicrobials and host defenses [23, 24].
QS systems and biofilm formation are crucial components in the development of acute and chronic infections, particularly for P. aeruginosa [25, 26], in which they play important roles in bacterial persistence and reduce sensitivity to antimicrobials [27]. Accordingly, molecules that affect the regulation of both QS mechanisms and biofilm formation could be powerful allies for conventional antibiotics in the struggle against bacterial infections [28, 29].
Recently, we demonstrated that a crude extract of Dalbergia trichocarpa bark inhibits the production of QS-dependent virulence factors in P. aeruginosa (pyocyanin, protease and elastase) as well as biofilm formation [30]. The present study describes the isolation, the identification and the biological characterization of the major bioactive compound in D. trichocarpa extract that inhibit both QS and biofilm formation without affecting bacterial growth.
Materials and Methods
Plant material
Stem bark samples of D. trichocarpa Baker. were collected in Madagascar from trees growing close to the city of Morondava (near the Kirindy forest, with the following GPS coordinates: 20° 04.120’ S 44° 39.250’ E, elevation 88 m). Collection authorization was delivered by MINENVEF (Ministry of Environment and Forest) authority represented by the Direction of Conservation, Biodiversity and Protected Area of Madagascar. Collection was carried out outside the protected Kirindy forest (tree cutting permission number 183/13/MEF/SG/DGF/DCB/SAP/SCB from 09/01/2013). Voucher specimen were deposited at FOFIFA (Centre National de la Recherche Appliquée au Développement Rural, BP 1690 Ampandrianomby 101 Antananarivo, Madagascar) and PBZT herbarium (Botanic and Zoologic Park of Tsimbazaza, Rue Fernand KASANGA Tsimbazaza 101 Antananarivo, Madagascar). D. trichocarpa Baker. is in the “Lower Risk/Least Concern” category according to the IUCN Red list of threatened Species (http://www.iucnredlist.org/details/36223/0).
Bacterial strains, plasmids, and culture conditions
PAO1 strain and its derivatives were grown (37°C, agitation 175 rpm) in LB-MOPS broth (50 mM, pH 7) supplemented with carbenicillin (300 μg mL-1) when appropriate. Plasmids (S1 Table) were used and introduced in PAO1 as previously described [31].
P. aeruginosa PAO1 mutant strains were obtained from the Transposon Mutant Collection (Department of Genome Sciences, University of Washington; http://www.gs.washington.edu/labs/manoil/libraryindex.htm) and include mutants 11174 (ΔPA1432, ΔlasI), 17281 (ΔPA1430, ΔlasR), 32454 (ΔPA3476, ΔrhlI) and 3452 (ΔPA3477, ΔrhlR) [32]. When required, the medium was supplemented with 10 μM (final) 3-oxo-C12-HSL or C4-HSL as described previously [33].
Chemicals
Naringenin, naringin and 4-nitro-pyridine-N-oxide (4-NPO) were purchased from Sigma-Aldrich and dissolved in 100% DMSO. Antimicrobial drugs (azithromycin and tobramycin) were purchased from TCI (Tokyo chemical industry Co. LTD, Japan) and dissolved in deionized water. The AHLs 3-oxo-C12-HSL and C4-HSL were purchased from Sigma-Aldrich and dissolved in 100% DMSO.
Chromatographic purification of the major bioactive compound from D. trichocarpa barks
Dried powdered samples of D. trichocarpa stem barks (10 kg) were macerated overnight at room temperature in 20 L n-hexane and extracted with 60 L n-hexane by percolation (1 liter for 1 h). The gathered n-hexane extracts were filtered on Whatman paper, evaporated under vacuum and the resulting residue (40 g) was stored at -20°C. The residue was dissolved in 30 mL of n-hexane, loaded onto a chromatography column (35 by 4 cm) filled with silica gel 60 F254 (63–200 μm / 70–230 mesh; Merck) and eluted with n-hexane and a step gradient of ethyl acetate (100:10 to 10:100) to afford 6 fractions (fractions F1 to F6) and then with ethyl acetate and a step gradient of methanol (100:10 to 10:100) to afford 3 fractions (fractions F7 to F9). The fractions were evaporated and stored at -20°C. The fraction most inhibitory of QS and biofilm was further fractionated by preparative HPLC using RP C18 column (Altima HP, 13 by 250 mm; 5μm) that was eluted with a gradient of water-acetonitrile (10:90 in 3 min, 10:90 to 0:100 in 4 min, 0:100 in 2 min, 0:100 to 10:90 in 1 min, 10:90 in 5 min). Subfractions were collected, monitoring at 300 nm, using Buchi fraction collector C-660 with SepacoreRecord software assistance, and evaporated for anti-QS/anti-biofilm activities. The active subfraction was further purified on prepHPLC with the same conditions until positive peak purity, as assessed by spectroscopy (diode array detection under ChemStation 9.0 software) and TLC (Silicagel RF254 Merck; mobile phase, Hexane-ethyl acetate [70–30]; detection: UV illumination (254 and 366 nm) and after developing by spraying with 10% (v/v) H2SO4 followed by heating at 110°C for 10 min).
Electrospray ionization mass spectrometry (ESI-MS) analysis and NMR spectroscopy of purified compound
The purified active compound (OALC) was analyzed by LC-ESI-MS with direct infusion into a Finnigan LCQ DUO mass spectrometer. The ESI parameters were as follows: solvent acetonitrile; concentration loaded 10 μg mL-1; negative ionization mode; nebulizer tip set at 250°C and 4.52 kV; cone voltage set at 5 kV; sheath gas (nitrogen) flow rate at 28 arbitrary units; collision energy at 70 eV; MS data were acquired in the m/z range from 50 to 2000. 1H- and 13C-NMR, COSY, NOESY, HSQC, and HMBC spectra were recorded on a Bruker Avance 400 NMR spectrometer. Standard pulse sequences and parameters were used for the NMR experiments and all chemical shifts were reported in parts per million (ppm, δ).
Gene expression and β-Galactosidase measurements
To monitor gene expression of QS-dependent (lasB and rhlA), QS-regulatory (lasR/I and rhlR/I), gacA and vfr genes, the β-galactosidase activity induced by reporter genes was measured using o-nitrophenyl-β-D-galactopyranoside [34, 35]. After growth in liquid LB-MOPS-Carbenicillin at 37°C and 175 rpm for 18 hours, PAO1 reporter strains were washed twice in fresh LB medium and resuspended in liquid LB-MOPS-Carbenicillin. PAO1 reporter strains inoculums (50 μl) were incubated (37°C with 175 r.p.m. agitation) for 18 hours in 1 mL LB-MOPS-Carbenicillin (initial A600nm of culture comprised between 0.020 and 0.025) supplemented with 10 μl of OALC dissolved in DMSO (200 μM) or 10 μl of DMSO (1%, v/v). Additionally, the flavanone naringenin, known as QS quencher [33], and its inactive glycoside (naringin) were used as positive and negative controls, respectively. After incubation, the bacterial density was assessed by spectrophotometry (A600nm) and the gene expression by the β-galactosidase assay.
For global gene transcription monitoring, a QS-independent gene, i.e. the isocitrate lyase-encoding aceA gene expression was also evaluated [36].
Rhamnolipids extraction and quantification
For rhamnolipids extraction, P. aeruginosa PAO1 was grown at 37°C with agitation at 175 rpm for 18 h in 1 mL LB-MOPS medium supplemented with OALC (200 μM), naringin (4 mM) or naringenin (4 mM) or DMSO (1%, v/v). Bacterial cultures were centrifuged (3200 × g, room temperature, 5 min) and 1 mL of cell-free supernatant (Filtre Ultrafree-CL filters Millipore) was mixed with 1 mL of ethyl acetate and vigorously vortexed. Phase separation was then realized by centrifugation in a tabletop centrifuge at maximum speed (1 min). The upper, rhamnolipid-containing phase was transferred to a new reaction tube. This procedure was repeated three times. Finally, the organic solvent was removed by evaporation in a vacuum centrifuge.
Rhamnolipids were quantified by a methylene-blue-based method as described by Pinzon and Ju, [37] with some modification. Briefly, the rhamnolipid extract of each sample was dissolved in 4 mL of chloroform and put in contact with a freshly prepared methylene blue solution (200 μL of a 1 g l-1 methylene blue and 4.9 mL of distilled water). The pH of this methylene blue aqueous solution is adjusted to 8.6 ± 0.2 (usually achieved by adding 15 μL of a 50 mM borax buffer). After being vigorously mixed for 4 minutes, the samples were left to stand for 15 min for complexation. One mL of the chloroform phase was transferred in a new Eppendorf tube and mixed by vortexing with 500 μl of HCl 0.2 N. Finally, 200 μl of the superior acid phase, containing a portion of the complexed methylene blue, was transferred in a 96-well microplate (Greiner clear) and the absorbance was measured at 638 nm with SpectraMax M2 device (Molecular Devices) against an HCl 0.2 N blank. The absorbance values were converted to rhamnolipids concentration using a calibration curve established by applying the same procedure to standard rhamnolipids solutions of different concentrations.
Homoserine lactone quantification
AHLs (C4-HSL and 3-oxo-C12-HSL) were extracted from PAO1 cultures and quantified by LC-ESI-MS as proposed by Makemson et al. [38]. P. aeruginosa PAO1 was grown at 37°C with agitation at 175 rpm for 18 h in 5 mL LB-MOPS medium supplemented with OALC (200μM), naringenin (4 mM) or naringin (4 mM) or DMSO (1%, v/v). Bacterial cultures were centrifuged (3220 × g, room temperature, 5 min) and supernatants (4 mL) were acidified with 80 μl glacial acetic acid prior to being extracted three times with ethyl acetate (4 mL). Ethyl acetate extracts were combined, evaporated to dryness and dissolved in 1 mL acidified ethyl acetate (0.1%, v/v, glacial acetic acid). For background measurement, supernatants (4 mL) were alkalinized with 80 μl 4 M NaOH before ethyl acetate extraction, hydrolyzed lactone rings being too polar to be extracted. ESI-MS quantification was done by direct infusion into a Finnigan LCQ DUO mass spectrometer under soft ionization conditions (positive ionization mode; nebulizer tip set at 250°C and 4.52 kV; cone voltage set at 5 kV; sheath gas (nitrogen) flow rate: 30 arbitrary units) that did not fragment the AHLs. Scans were averaged over 1 min. The peak intensities for C4-HSL (pseudomolecular ion, m/z = 172; ammonium adduct, m/z = 189; sodium adduct, m/z = 194; solvent adduct, m/z = 260) and 3-oxo-C12-HSL (pseudomolecular ion, m/z = 298; ammonium adduct, m/z = 315; sodium adduct, m/z = 320; solvent adduct, m/z = 386) were combined and converted to concentrations by using a standard curve generated from the pure compounds. Background readings from hydrolyzed samples extracted with ethyl acetate were subtracted from those of the acid-extracted bacterial cultures before conversion. To evaluate an eventual chemical-modulation activity of OALC, LB-MOPS medium supplemented with OALC and/or exogenous AHLs (3-oxo-C-12HSL and C4-HSL) were incubated for 18h and AHLs have been extracted following the same procedure.
Quantitative analysis of pyocyanin and elastase production by P. aeruginosa PAO1
The production of pyocyanin and elastase was assessed according to previously described procedures [39, 40]. P. aeruginosa PAO1 or mutant strains were grown for 18 h in liquid LB-MOPS (supplemented with 60 μg mL-1 tetracycline for mutant strains). PAO1 cell suspension (50 μl) was added to 1 mL of LB-MOPS (starting A600nm ranged between 0.02 and 0.025) supplemented with 10 μl of OALC dissolved in DMSO (200 μM) or 10 μl of DMSO (1%, v/v) or naringenin (4 mM) or naringin (4 mM). When required, the medium was supplemented with 10 μM of 3-oxo-C12-HSL or C4-HSL as described previously [33]. After 18 h of growth, samples were taken to assess growth (A600nm) and pyocyanin production. The LasB elastase production was assessed through the measurement of elastase activity using elastin-Congo Red [40].
Assessment of bacterial growth
Relative growth of P. aeruginosa PAO1 after 18 hours in the presence of OALC was evaluated by measuring the cell density at A600nm with a SpectraMax M2 device (Molecular Devices). The effect of OALC on P. aeruginosa PAO1 growth kinetic was evaluated by evaluating PAO1 cell density (A600nm) over 22 hours culture, confirmed by cell counting (colony-forming units, C.F.U) at times 8 and 18 h.
Motility assays
The swarming motility was examined using LB agar plate described previously [41]. Briefly, LB agar (0.6%) medium supplemented with glutamate (0.05%) and glucose (0.2%) was autoclaved for sterilization. Sterilized medium was cooled at temperature between 45–50°C and then supplemented (DMSO 1% or OALC at 200 μM or naringenin at 4 mM or naringin at 4 mM) before being poured into compartmented Petri dishes. Gelled plates were inoculated at their center with 5 μl of a bacterial culture of PAO1 cells diluted to a turbidity of 1 at 600 nm and placed at 37°C when inoculums spots are dry. Bacteria spreading from the inoculation spot were measured after 24 hours. The twitching motility was assayed as previously described [42] with slight modification. Briefly, plates with LB agar (1%) supplemented (DMSO 1% or OALC at 200 μM or naringenin at 4mM or naringin at 4mM) poured to an average depth of 3 mm were prepared and dried briefly. A hole (about 1mm diameter) was dug in the center of each compartment through the agar and 5 μl of P. aeruginosa PAO1 cells diluted to a turbidity of 1 at 600 nm were spotted inside the hole, dried briefly and incubated at 37°C for 48 hours. After the incubation period, bacteria spreading between the agar and the bottom of the petri dish were measured. For diameters measurement, the agar was discarded from petri dish and twitching motility zones were easily visualized by staining for 1 minute with 0.1% (w/v) of crystal violet as proposed by Darzins [43].
Biofilm quantification and synergistic activity with tobramycin
P. aeruginosa PAO1 was grown overnight in LB medium at 37°C with agitation. After growth, the culture of P. aeruginosa PAO1 was diluted with Biofilm Broth (BB) medium as described by Khalilzadeh et al. [44] and 25 μl of the diluted culture was added to 470 μl of BB medium (initial A600nm of culture comprised between 0.14 and 0.16) supplemented with 5 μl of DMSO (1%, v/v) or OALC (200 μM) or naringenin (4mM) or naringin (4mM). Planktonic bacteria were transferred in sterile tube and assessed for cell counting (colony-forming units, C.F.U). Adherent biofilms were washed three times with water (2mL) and fixed with 2 mL of methanol (99%). After 15 min, the methanol was discarded, and the plates were dried at room temperature. Crystal violet (0.1% in water) was then added to each well (2 mL/well), and the plates were incubated for 30 min at room temperature. Crystal violet was then discarded, and stained biofilms were washed three times with 1 mL of water. Acetic acid (33% in water) was added to the stained biofilms (2 mL) in order to solubilize the crystal violet, and the absorbance of the solution was measured at 590 nm with a SpectraMax M2 device (Molecular Devices).
The biofilm formation by PAO1 cells was also examined in glass coverslips cultures by fluorescence microscopy. Two distinct assays were adopted in order to assess the effects of compounds in biofilm development and in one-day-old biofilm. In both cases, the bactericidal activities of tobramycin in one-day-old biofilm-encapsulated PAO1 cells was also assessed. Tobramycin was chosen because it has been shown that QS inhibition greatly enhances the sensitivity of P. aeruginosa to this antibiotic and increases clearance of P. aeruginosa in a foreign-body infection model [28, 45]. First assay follows the same culture conditions as described above. After 24 h incubation, tobramycin (100 μg mL-1) was added to 1-day-old treated biofilms. The biofilm development and bacterial viability in biofilms were assessed using the LIVE/DEAD baclight bacterial viability kit (Invitrogen, Molecular probes). The growth medium was removed and replaced by 500 mL of a solution of SYTO 9 and propidium iodide diluted 400 fold in BB medium. Biofilms were incubated for 15 min and PAO1 cells were examined using a Leica DM IRE2 inverted fluorescence microscope coupled to a CCD camera (Leica DC350 FX) and equipped with FITC and Texas red filters. To estimate the % viability of biofilm-encapsulated bacteria for each treatment, the glass coverslip was submerged in 2 mL of PBS solution and sonicated (WVR Ultrasonic cleaner, HF45KHz, 80W) for 1 min in order to unbind the biofilm. The collected biofilm suspension was then assessed for viability using LIVE/DEAD baclight bacterial viability kit (Invitrogen, Molecular probes) following fluorescence microplate reader protocols as described by the manufacturer. The integrated intensities of the green (530 nm) and red (630 nm) emission of suspensions excited at 485 nm were acquired using SpectraMax M2 device, and the green/red fluorescence ratios (Ratio G/R) were calculated and reported to the linear curve obtained from the relationship between % live bacteria and Ratio G/R of biofilm-encapsulated PAO1 cells grown without tobramycin.
For the second assay, PAO1 cells were grown statically in BB medium for 24 hours at 37°C in 24-well polystyrene plates to form biofilm. Tested molecules as described above and/or tobramycin (100 μg mL-1) were added and incubated for a further 24 hours and the biofilm development and bacterial viability in biofilms were assessed as described for the first assay.
Total extracellular polysaccharides and alginate quantification
For extracellular polysaccharides extraction, the method using ethanol was followed as described by Gong et al. [46]. Briefly, P. aeruginosa PAO1 was grown at 37°C with agitation at 175 rpm for 18 h in 5 mL LB-MOPS medium supplemented with OALC (200 μM), naringin or naringenin (4 mM) or DMSO (1%, v/v). The bacterial culture was centrifuged (3200 × g, room temperature, 5 min) and the supernatant discarded. The freshly harvested cell pellet was resuspended in 10 mL 0.22% formaldehyde (ACS grade, Fisher Scientific) in 8.5% sodium chloride for 2 h in a 4°C incubator. Following the exposure to formaldehyde, the suspension was centrifuged (3200 × g, 4°C, 15 min) and the resulting pellet containing the polysaccharides was resuspended in 10 mL deionized (DI) water (Millipore, Milli-Q Academia). Then the suspension was centrifuged again (3200 × g, 4°C, 15 min) to rinse away any remaining cellular material, the pellet was collected, weighted, resuspended in DI water (50 μL per mg of pellet), sonicated for 3 min (460 = H Elma Transsonic Lab-Line Instruments, Germany) and centrifuged once more at 3200 × g, 4°C for 15 min (Eppendorf Centrifuge 5810R). This polysaccharides pellet was suspended in 5 mL 10−2 M KCl and 10 mL pure and cold ethanol, incubated overnight at 4°C to reprecipitate the polysaccharides that were centrifuged (3200 × g, 4°C, 20 min). After decantation, the purified pellet was suspended in 10 mL DI water and the total amount of carbohydrates was evaluated with the Phenol-Sulfuric Acid (PSA) method [47]. Two mL of this polysaccharides solution were added with 50 μL of a 80% phenol solution (Fisher Scientific) and, carefully, 5 mL of 95% sulfuric acid (Fisher Scientific), incubated, 30 min at 25°C, 4 h at room temperature (22–25°C) and measured at 480 nm with SpectraMax M2 device (Molecular Devices) referring to glucose as a standard [48].
Alginate was quantified by a slightly modified carbazole-based method that detects uronic acids [49]. One mL overnight grown P. aeruginosa culture was mixed with 1 mL of 0.85% NaCl and the A600 of the solution was determined after 1 min vortex. After elimination of bacteria (13 000 x g, 60 min), the alginate present in 1 mL of the supernatant was precipitated by addition of 1 mL 2% cetyl pyridinium chloride and collected (13 000 × g, 20 min). The pellet was dissolved in 1 M NaCl, precipitated again with 1 mL of cold (-20°C) isopropanol, centrifuged (13 000 g, 20 min, 4°C), resuspended in 1 mL saline and stored at 4°C. Fifty μl of serial dilutions of standard (sodium alginate 0.1–1 mg mL-1) or sample were added with 200 μl of 25 mM sodium tetraborate in concentrated sulfuric acid, heated for 10 min at 100°C, cooled at room temperature for 15 min and carefully added with 50 μl of 0.125% carbazole in absolute ethanol. After heating at 100°C for 10 min and cooling at room temperature for 15 min, 300 μl of the reaction product were transferred into an appropriate cuvette and measured at a wavelength of 550 nm.
C. elegans paralytic killing and toxicity assay
Viability of adult nematodes deposited on the lawn of PAO1 was assessed as described previously with some modification [50, 51]. P. aeruginosa PAO1 (virulent strain), ΔPA1430, (ΔlasR) and ΔPA3477 (ΔrhlR) (reduced virulent strains) were grown overnight in LB and then diluted 100-fold into fresh broth. Brain Heart Infusion agar plates containing either DMSO 1%, OALC (200 μM), naringenin (4 mM), naringin (4 mM) or 4-NPO (100 μM) were spread with 400 μl of diluted culture and then incubated at 37°C for 24 h to form lawns of bacteria. Synchronized culture L4 nematodes or adult wild-type nematodes (From University of Minnesota), obtained as previously described [52], were washed off stock plates and suspended in a minimal volume of PBS buffer (pH 6.5). One hundred μl of nematodes suspension were placed onto the P. aeruginosa lawns and incubated at 20°C; the droplets dried within 30 min and deposited the nematodes on the lawn. Likewise, nematodes free of P. aeruginosa were deposited on plates containing OALC or naringenin or DMSO to evaluate an eventual toxicity. Plates were then sealed with parafilm and incubated at 20°C. After 4 h, deposited nematodes were retrieved with PBS buffer (pH 6.5) and the obtained worm suspension was transferred into a 15-mL tube and centrifuged (1300 rpm, 2 min), rinsed twice with 5 mL PBS and resuspended in 1 mL PBS for preparing the fluorescence revelation of dead worms as described elsewhere [53]. Briefly, washed-worm suspension was labelled by adding 200 μl of a 5(6)-carboxyfluorescein diacetate (CFDA) working solution and leaving for 30 min at room temperature in the dark. After centrifugation (1300 rpm, 2 min) and washing with 5mL PBS to eliminate the excess of fluoresceine, the pellet was resuspended in 1 mL PBS and divided into 200 μl aliquots containing around 20–40 worms. The proportion of dead worms was then measured by visual counting (triplicate counting) in fluorescence microscopy.
Statistics
All experiments were performed in quintuplicate and repeated in three independent assays. The data were statistically analyzed by conducting Student’s t tests and a p value ≤ 0.01 was considered as being significant.
Results
Oleanolic aldehyde coumarate isolated from D. trichocarpa bark extract reduces the expression of QS-regulated lasB and rhlA genes
To identify the QS inhibitory (QSI) compound(s) occurring in the D. trichocarpa bark (DTB) extract, the chromatographic fractionation was bio-guided by quantification of lasB and rhlA gene expression as well as biofilm formation in P. aeruginosa PAO1. The procedures and results that led to the isolation of the active compound are detailed in S1 Text and S1 Fig. The chemical structure of the isolated active compound was elucidated through spectroscopic analyzes, including UV, mass and NMR spectral data which are detailed in S2 Text, S2 and S3 Figs, leading to its identification as a 3β-hydroxyolean-12-en-28-al 3-p-coumarate or oleanolic aldehyde coumarate (OALC, MW: 586.52, C39H54O4; Fig 1 and S2 Table).
[Figure omitted. See PDF.]
Fig 1. Chemical structure of the bioactive compound assigned as 3β-hydroxyolean-12-en-28-al 3-p-coumarate (oleanolic aldehyde coumarate, OALC).
https://doi.org/10.1371/journal.pone.0132791.g001
The effect of OALC on lasB and rhlA expression was then evaluated at different concentrations (from 50 to 200 μM). As shown in S4A and S4B Fig, significant reduction of the expression of both genes is observed from 150 μM of OALC. For instance, at 200 μM of OALC 61 ± 5% of inhibition for lasB and 69 ± 5% of inhibition for rhlA was recorded. To monitor the effect of OALC on global gene transcription, a QS-independent gene, i.e. the isocitrate lyase-encoding aceA gene expression was evaluated (see experimental procedures for details). As shown in S4C Fig, aceA expression as well as bacterial growth were not affected by OALC at the tested concentrations. Consequently, as more than 50% inhibition in QS gene expression was recorded in presence of 200 μM of OALC, this concentration was used in all further experiments. Higher concentrations were not assessed due to limited quantity of purified OALC.
To evaluate the impact of OALC on P. aeruginosa PAO1 growth and viability, growth kinetics and C.F.U. measurements were recorded in the presence of 200 μM of OALC. As shown in S5 Fig, P. aeruginosa growth kinetics and viability were not significantly affected by OALC as compared to the DMSO treatment; this was shown by both culture turbidity measurements (S5A Fig) and C.F.U. quantifications after 8 and 18 hours of growth (S5B and S5C Fig). This result suggests that the decrease in QS gene expression and biofilm formation were not due to a drop in cell viability.
OALC reduces the production of QS-dependent virulence factors (pyocyanin, elastase and rhamnolipids) as well as native AHLs production in P. aeruginosa PAO1
As lasB and rhlA expressions are reduced in PAO1 cells treated with OALC, this could be reflected in the production of associated-virulence factors. Thus, we assessed the effect of OALC (at 200 μM) on the production of three QS-dependent virulence factors, i.e. rhamnolipids, pyocyanin and elastase. As shown in Fig 2, a drastic inhibition of the production of rhamnolipids (75 ± 4% of inhibition; Fig 2A) and pyocyanin (64 ± 3% of inhibition; Fig 2B) was observed when PAO1 strains were grown in the presence of OALC compared to PAO1 strains grown with DMSO. Additionally, OALC also reduced elastase production (19 ± 4% of inhibition; Fig 2C) and OALC did not degrade elastine-Congo red in bacteria-free tests (data not shown).
[Figure omitted. See PDF.]
Fig 2. Effect of OALC on virulence factors and acylhomoserine lactones production in P. aeruginosa PAO1.
(A) rhamnolipids production, (B) pyocyanin production, (C) Elastase production. The cell density of the bacteria was assessed at 600 nm and elastase production was assessed via an elastolysis assay and calculated as the ratio between A495 and A600. The rhamnolipids production was measured using methylene-blue-based method and expressed in μg mL-1. Pyocyanin was extracted, quantified by absorbance measurements at 380 nm and calculated as the ratio between A380 and A600. (D) Quantification of N-(3-oxododecanoyl)-L-homoserine lactone (3-oxo-C12-HSL; grey bar) and N-butanoyl-L-homoserine lactone (C4-HSL; clear bar) produced by PAO1 cells. Acylhomoserine lactones were extracted and quantified by mass spectrometry. Error bars represent the standard errors of the means and all experiments were performed in quintuplicate with three independent assays and asterisks indicate samples that are significantly different from the DMSO controls (Student’s t-tests; P ≤ 0.01). Naringenin (Nar) and naringin (Nin) were used as a quorum sensing inhibitor control and negative control, respectively.
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The expression of the las- and rhl-dependent virulence factor genes is positively controlled by the transcription factor complexes LasR/3-oxo-C-12-HSL and RhlR/C4-HSL, respectively [9]. Thus, the observed reduction in the expression of lasB and rhlA genes induced by OALC could be linked to a reduction of 3-oxo-C12-HSL and C4-HSL levels in culture media. As shown in Fig 2D, OALC significantly reduced the concentrations of both auto-inducers after 18 h of growth, by 3- and 4-fold for C4-HSL and 3-oxo-C12-HSL, respectively. To address the matter of whether OALC reacts directly with the AHL released in culture medium, LB-MOPS medium supplemented with OALC and/or exogenous AHLs (3-oxo-C-12HSL and C4-HSL) have been incubated for 18h and AHLs were then extracted and quantified (see experimental procedures for details). No significant difference in extracted AHLs was observed, suggesting the absence of reactivity towards AHLs (data not shown). At this stage, reduction of native AHLs in culture media is presumably linked to a direct or indirect inhibition of AHLs production by OALC.
To address the matter of whether AHLs supply could restore the production of QS-virulence factors in the presence of OALC, 3-oxo-C12-HSL or C4-HSL were added exogenously to OALC-treated PAO1 cells. As shown in S6 Fig, the addition of 3-oxo-C12-HSL or C4-HSL at 10 μM (see experimental procedures for details) did not restore the production of pyocyanin or elastase in OALC-treated wild-type PAO1 cells (S6A and S6B Fig). The same experiment was performed with the ΔPA1432 and ΔPA3476 mutant strains (which lack functional lasI and rhlI synthetase genes, respectively) to avoid interference with native AHLs (S6C Fig). The exogenous addition of 3-oxo-C12-HSL to the ΔPA1432 strain significantly increased elastase production, but adding OALC reduced this production to the base level (S6C Fig), confirming that an exogenous supply of AHLs is not sufficient to compensate the effect of OALC. As shown in S6D Fig, the ΔPA3476 mutant was unable to produce pyocyanin unless C4-HSL was exogenously supplied (while 3-oxo-C12-HSL had no effect). Similarly to ΔlasI strain, when OALC was added to C4-HSL-induced ΔrhlI cells, the level of pyocyanin production was three-fold lower than that observed when C4-HSL alone was added (S6D Fig). These data, consistent with those obtained on the wild type strain PAO1 supplemented with exogenous AHLs, confirm that the reduction of native AHLs induced by OALC is not compensated by exogenous AHLs supply. All together these data indicate that OALC could exert its effect beyond AHLs synthesis in the QS pathways. To further document this hypothesis, the expression of QS regulatory genes (lasI/R and rhlI/R) and two global activator genes (gacA and vfr) was investigated.
OALC affects the expression of lasI/R, rhlI/R and the global activator gacA
As shown in Fig 3A and 3B, OALC significantly reduces (p ≤ 0.01) the expression of the rhlI and lasI genes (39 ± 3% and 33 ± 5% of inhibition, respectively). Similarly, OALC significantly reduces the expression of lasR and rhlR genes (35 ± 3% and 50 ± 3% of inhibition, respectively). In the hierarchical P. aeruginosa-QS cascade, the global activator GacA and Vfr are positioned upstream and exert a positive effect on the transcriptional regulators LasR and RhlR [19, 20]. In this respect, the effect of OALC on gacA and vfr genes expression was therefore investigated. As the effect of naringenin on the expression of the global activator genes gacA and vfr had not been previously evaluated, azithromycin (1 μg mL-1 final concentration) was preferred as positive inhibitory control [54]. As shown in Fig 3C, OALC exhibits a small but significant inhibitory effect on gacA expression (16 ± 4% of inhibition; P ≤ 0.01) but no effect on vfr expression.
[Figure omitted. See PDF.]
Fig 3. Effect of OALC on QS genes (lasI/R and rhlI/R) and global activator genes (gacA and vfr) expression in P. aeruginosa PAO1.
(A) Effect of OALC on lasR (grey bar) and lasI (clear bar) expression following 18 hours of growth. (B) Effect of OALC on rhlR (grey bar) and rhlI (clear bar) expression following 18 hours of growth. (C) Effect of OALC on gacA (grey bar) and vfr (clear bar) expression following 18 hours of growth. Gene expression was measured as the β-galactosidase activity of the lacZ gene fusions and expressed in Miller units. Error bars represent the standard errors of the means; all experiments were performed in quintuplicate with three independent assays and asterisks indicate samples that are significantly different from the DMSO (Student’s t-tests; P ≤ 0.01).
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OALC affects biofilm formation in P. aeruginosa PAO1
As evidenced by the bio-guided chromatographic fractionation (see S1 Fig), OALC inhibits biofilm formation by P. aeruginosa PAO1. To further detail the effect of OALC on biofilm formation, its effect was compared in two growth media, a minimum and a complex medium (See experimental procedures) as biofilm development is nutritionally conditioned [55]. As shown in Fig 4A, OALC significantly reduced the biomass of the PAO1 biofilm in both minimal and complex media (44 ± 4% and 36 ± 5%, respectively). Additionally, in minimal media, a significant increase of planktonic bacteria is recorded compared to DMSO (Fig 4B), suggesting that OALC promotes planktonic bacteria lifestyle instead of biofilm.
[Figure omitted. See PDF.]
Fig 4. Effect of OALC on biofilm formation by P. aeruginosa.
(A) Quantification of biofilm formation by P. aeruginosa PAO1 grown in minimal (grey bar) and complex media (clear bar) after static incubation at 37°C for 24 hours. (B) Quantification of biofilm formation by P. aeruginosa grown in in minimal media (grey bar) and C.F.U. measurement (clear bar) of planktonic bacteria after static incubation at 37°C for 24 hours. Biofilm formation was quantified by crystal violet staining and measured at A590nm. The cell density of the bacteria was assessed at 600 nm. Error bars represent the standard errors of the means; all experiments were performed in quintuplicate with three independent assays and asterisks indicate samples that are significantly different from the DMSO (Student’s t-tests; P ≤ 0.01).
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Visualization of P. aeruginosa biofilm by fluorescence microscopy using SYTO-9 and propridium iodide (to stain live and dead cells, respectively) indicated that PAO1 grown for 24 hours in static condition (and with DMSO) forms a thick and homogenous biofilm layer on coverslips with good cell-to-cell connections interspaced by uncolonized surfaces (Fig 5A). Similar biofilms were observed in cells treated with the negative control naringin, although confluent bacterial biofilms were visually less thick as observed with fluorescence microscopy. By contrast, OALC- and naringenin-treated PAO1 cells failed to establish compact cell-to-cell attachment resulting in a reduction of microcolonies confluence (Fig 5A). Interestingly, when applied to one day-old pre-formed biofilm, both OALC and naringenin disrupted the architecture of PAO1 biofilm, as shown by the presence of aggregates and less confluent microcolonies (Fig 5B). On the contrary, application of DMSO- and naringin on one-day-old biofilms had no impact (Fig 5). This result suggests that important components for PAO1 biofilm formation and structure maintenance are impaired in the presence of OALC.
[Figure omitted. See PDF.]
Fig 5. PAO1 biofilm phenotypes as affected by DMSO, naringin, naringenin or OALC.
(A) Fluorescence microscopy images of PAO1 cells incubated statically at 37°C for 24 hours. Cells were visualized after staining with SYTO-9 (green fluorescence for living bacteria) and propidium iodide (red fluorescence for dead bacteria) furnished in the LIVE/DEAD BacLight kit. (B) Fluorescence microscopic images of biofilm formation by PAO1 cells incubated for 24 hours and then treated for 24 hours with DMSO, naringin, naringenin or OALC. Fluorescence microscopy was achieved by using a Leica DM IRE2 inverted fluorescence microscope using a 40x objective lens and images were false-colored and assembled using Adobe Photoshop.
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Major PAO1 phenotypes contributing to biofilm formation, including swarming, twitching motilities and extracellular polysaccharides, are affected by OALC
To invade surfaces, P. aeruginosa uses swarming and twitching motilities; both processes are under QS regulation and contribute to the initial stages of biofilm formation and architecture [56–58]. As shown in Fig 6, PAO1 swarming was significantly affected when grown onto LB agar supplemented with OALC or naringenin but not when DMSO and naringin were supplemented to the medium (Fig 6A). This reduction of bacterial motilities by OALC could contribute to reducing their ability to form confluent microcolonies (Fig 5A).
[Figure omitted. See PDF.]
Fig 6. Effect of OALC on P. aeruginosa PAO1 motilities.
(A) Swarming motility of P. aeruginosa PAO1 onto LB agar (0.6%) supplemented with glutamate (0.05%), glucose (0.2%) and DMSO (1%) or OALC (200μM final concentration), naringenin (Nar, 4 mM final concentration) or naringin (Nin, 4 mM final concentration). After incubation at 37°C for 24 hours, the zones of migration (down) from the point of inoculation were measured (up) for each condition. (B) Twitching motility of P. aeruginosa PAO1 onto LB agar (1%) supplemented with DMSO (1%), OALC (200μM final concentration), Nar (4 mM final concentration) or Nin (4 mM final concentration). The twitching zones were stained (down) and their diameters (up) measured after incubation at 37°C for 48 h. Error bars represent the standard errors of the means and all experiments were performed in quintuplicate with three independent assays and asterisks indicate samples that are significantly different from the DMSO (Student’s t-tests; P ≤ 0.01).
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Fluorescence microscopy analyses revealed distinct micro-morphological alterations of the adherent bacteria and biofilm matrix after OALC and naringenin treatment, suggesting the disruption of matrix components (Fig 5). Consistently, the amount of extracellular polysaccharides produced by PAO1 after 24 hours of growth was reduced in OALC- and naringenin-treated PAO1 cells (40 ± 4% and 66 ± 5%, respectively) compared to the DMSO treatment (Fig 7A). However, the production of alginate, an acidic polysaccharide composed of non-repeating subunits of D-mannuronic and L-guluronic acid [59], was not significantly different compared to the DMSO treatment (Fig 7B). Thus, the global reduction of extracellular polysaccharides is presumably linked to reductions in Pel and/or Psl (polysaccharide synthesis locus) polysaccharides, a reduction that could negatively impact the biofilm structures of PAO1.
[Figure omitted. See PDF.]
Fig 7. Effect of OALC on extracellular polysaccharides production by P. aeruginosa PAO1.
(A) Quantification of total extracellular polysaccharides. The cell density of the bacteria was assessed at 600nm and extracellular polysaccharides production was measured using Phenol-Sulfuric Acid (PSA) method and expressed in μg mL-1 with glucose as standard. (B) Quantification of alginate. The cell density of the bacteria was assessed at 600nm and alginate production was measured using carbazole method and expressed in μg mL-1 with sodium alginate as standard. Error bars represent the standard errors of the means; all experiments were performed in quintuplicate with three independent assays and asterisks indicate samples that are significantly different from the DMSO (Student’s t-tests; P ≤ 0.01). Naringenin (Nar) and naringin (Nin) both at 4 mM final concentration were used as quorum sensing inhibitor positive and negative controls, respectively.
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OALC exhibits antibiotic-synergizing activities in biofilm
Since OALC affects both biofilm formation and structure maintenance (Fig 5) as well as EPS production (Fig 7), it is tempting to evaluate the protective ability of biofilm matrix treated with OALC against environmental aggressions such as antibiotics. For that, tobramycin has been selected because it is widely used to treat acute P. aeruginosa exacerbations in patients with cystic fibrosis [60] but appears less effective in biofilm-encapsulated P. aeruginosa compared to their planktonic counterparts [61]. Moreover, EPS has been demonstrated to be a barrier for antibiotic attacks by limiting the penetration of tobramycin [62, 63]. As shown in Fig 8, OALC in association with tobramycin significantly increased the effectiveness of the antibiotic against biofilm-encapsulated bacteria. Indeed, tobramycin introduced at 100 μg mL-1 in one day-old biofilm-encapsulated PAO1 cells was found to kill 90 ± 5% of OALC-treated biofilm cells (ie, OALC was introduced during the initial growth of PAO1 to form one day-old biofilm) (Fig 8A), whereas tobramycin alone could kill only 36 ± 4% (Fig 8B). Similar results were observed for the naringenin-tobramycin treatment (86 ± 5% of dead cells; Fig 8C), whereas the association of tobramycin with DMSO (Fig 8D) or naringin (Fig 8E) did not exhibit significant bactericidal effect (45 ± 5% and 40 ± 3%, respectively) compared to tobramycin alone. Although less efficient, this synergistic effect was also manifest when OALC-tobramycin are added to one day-old biofilm cultures (76 ± 3% of dead cells) contrarily to the associations tobramycin-DMSO and tobramycin-naringin (40 ± 4% and 44± 6%, respectively; Fig 9). These results suggest an improvement of antibiotic diffusion/penetration through the biofilm matrix in the presence of OALC which is correlated with the decrease of EPS production and biofilm architecture disruption induced by OALC.
[Figure omitted. See PDF.]
Fig 8. Synergistic activity of OALC with tobramycin against biofilm-encapsulated P. aeruginosa PAO1.
PAO1 cells were incubated statically for 24 hours in the presence of DMSO, naringin (4 mM), naringenin (4 mM) or OALC (200 μM) and then treated for 24 hours with tobramycin (100 μg mL-1). (A) OALC + tobramycin, (B) tobramycin, (C) naringenin + tobramycin, (D) DMSO + tobramycin, (E) naringin + tobramycin. Assessment of bacterial viability and microscopy were performed as in Fig 6. (F) Quantification of bacterial viability. Error bars represent the standard errors of the means; all experiments were performed in quintuplicate with three independent assays and asterisks indicate samples that are significantly different from the DMSO (Student’s t-tests; P ≤ 0.01).
https://doi.org/10.1371/journal.pone.0132791.g008
[Figure omitted. See PDF.]
Fig 9. Synergistic activity of OALC with tobramycin against biofilm-encapsulated P. aeruginosa PAO1.
PAO1 cells were incubated statically for 24 hours and then treated for 24 hours with tobramycin (100 μg mL-1) and DMSO, naringin (4 mM), naringenin (4 mM) or OALC (200 μM final concentration). (A) OALC + tobramycin, (B) tobramycin, (C) naringenin + tobramycin, (D) DMSO + tobramycin, (E) naringin + tobramycin. Assessment of bacterial viability and microscopy were performed as in Fig 6. (F) Quantification of bacterial viability. Error bars represent the standard errors of the means; all experiments were performed in quintuplicate with three independent assays and asterisks indicate samples that are significantly different from the DMSO (Student’s t-tests; P ≤ 0.01).
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OALC reduces paralytic killing activity of P. aeruginosa PAO1 on Caenorhabditis elegans
P. aeruginosa PAO1 strains are known to cause death of C. elegans by neuromuscular paralysis [64], which has been demonstrated to be LasR-dependent [65]. Thus, the success of OALC in affecting P. aeruginosa PAO1 QS systems suggested that this molecule might also reduce C. elegans mortality in a PAO1-nematode model. Synchronized culture of wild type L4 adult nematodes obtained as described previously [52] (See experimental procedures for details) were therefore deposited on a lawn of PAO1 pre-treated with OALC, naringenin, naringin, DMSO or 4-NPO (a reference QSI agent) [50]. After 4 hours of incubation, dead worms were counted following fluorescence revelation as previously described [51, 53]. As shown in S7A Fig, more than 80% of the worms died within 4 hours onto plates containing PAO1 conditioned with DMSO 1%. When treated with 4-NPO (100 μM) or with OALC (200 μM), the wild-type PAO1 strain could kill only 27 ± 2% and 52 ± 2% of the worms, respectively. Similar results were observed with naringenin (52 ± 4% of dead worms). QS-defective strains ΔlasR and ΔrhlR pre-treated in the different conditions induce only 20 to 30% of nematode death after 4 hours (S7B and S7C Fig). However, naringenin at 4 mM and OALC at 300 μM (not 200μM) turned out to be toxic to C. elegans, with a death count of about 60 to 65% (S7D Fig).
Discussion
Antimicrobial resistance is undoubtedly a growing worldwide public health threat so that the WHO foresees the emergence of a ‘post-antibiotic’ era during the 21st century in which common infections and minor injuries will have a dramatic impact on human death toll [2, 66]. Infection control using strategies inhibiting bacterial virulence and/or biofilm formation are increasingly explored as anti-pathogenic approaches because they are thought to minimize the selection pressure and the concomitant emergence of resistances experienced with strategies targeting basic cell mechanisms and leading to pathogen’s death [29, 67]. In the case of P. aeruginosa, several chemical structures (synthetic and natural) have been reported so far to present, at the same time, anti-QS, anti-biofilm and in-biofilm antibiotic-synergizing activities [68]. The hemisynthetic compound azithromycin (AZM, a macrolide antibiotic) was found to present both QS and biofilm inhibitory effects in P. aeruginosa when used at sub-bactericidal concentration [2.67 μM] [69]. A number of natural compounds have also been demonstrated to affect QS-controlled gene expression in P. aeruginosa and to reduce biofilm production; these include, among recently reported, 6-gingerol [at 10 μM] (a pungent oil of fresh ginger) [70], eugenol from clove [at 50 μM][71], ajoene [at 100 μM] (an allyl sulfide from garlic) [45], S-phenyl-L-cysteine sulfoxide [at 1 mM] [72] and some flavonoids (the flavan-3-ol catechin [at 4 mM] [35] from Combretum albiflorum and naringenin [at 4 mM] [33]). Herein, OALC exerts its activity at 200 μM in the range of other compounds reported elsewhere.
In the present report, the bio-guided fractionation of D. trichocarpa bark extract led to the isolation and identification of an oleanolic aldehyde coumarate (3β-hydroxyolean-12-en-28-al 3-p-coumarate or OALC) as a novel QSI and anti-biofilm compound without bactericidal effect. D. trichocarpa is traditionally used along the west coast of Madagascar as local medicine to treat various ailments such as laryngitis, diarrhea and rheumatic pains [73]. Besides, the antimicrobial activity of extracts from Dalbergia species including D. parviflora Roxb. and D. horrida Dennst. has also been reported and was mainly attributed to flavanone and isoflavone derivatives [74–76]. To the best of our knowledge, this is the first report of the occurrence of OALC in any genus/species of plant or other organisms. However, a closely related derivative, oleanolic acid coumarate, has been previously isolated from Jatropha curcas L. [77] and Hippophae rhamnoides L. [78] and was shown to present an antimycobacterial (Mycobacterium tuberculosis) activity [79]. Besides, Hu et al. [80] demonstrated that a closely related compound, 20β-hydroxyursolic acid coumarate, isolated from leaves of Diospyros dendo inhibits biofilm formation in P. aeruginosa PAO1; though, this compound was not screened for anti-QS activities.
In P. aeruginosa PAO1, OALC at 200 μM seems to display a large number of biological activities including QSI and anti-biofilm activities that implies multiple cellular targets. Indeed, OALC inhibits QS-regulatory (lasI/R and rhlI/R), QS-regulated (lasB and rhlA), global activator gacA genes expression (Fig 3) and alters biofilm formation and maintenance (Figs 4 and 5). Multiple studies demonstrate that QS systems contribute to the ability of bacteria to form biofilms [81, 82]; for instance, P. aeruginosa defective in QS are compromised in their ability to form biofilms [81, 83]. In the case of OALC, one can assume an indirect link between QS and biofilm formation through the control of essential components such as polysaccharides (Fig 7) and rhamnolipids (Fig 2) production, as well as swarming and twitching motility (Fig 6), that are all negatively regulated by OALC. Indeed, inactivation of the rhlA gene (crucial for rhamnolipids biosynthesis) causes an inhibition of swarming motility and reduces twitching motility [41, 84]. In addition, it has been reported that P. aeruginosa strains limited in swarming motility form biofilms containing non-confluent cell aggregates [58], a phenotype similar to that induced in OALC-treated PAO1 biofilm (Fig 5). In the same line, twitching motility, which has also been shown to be regulated by the rhl system [85], is necessary for the assembly of a P. aeruginosa cell monolayer into microcolonies [86]. Moreover, mutants deficient in rhamnolipids synthesis fail to maintain open channels, which are necessary for distribution of nutrients and oxygen within the biofilm matrix [87]. In addition, rhamnolipids are involved in microbial cell adhesion and biofilm development [88]. A reduction of rhamnolipids production as suggested by the down regulation of rhlA expression by OALC, might result in a decreased development or a disruption of developing biofilms. Thus, rhamnolipids reduction in OALC-treated PAO1 (Fig 2) as well as failure in swarming and twitching motilities (Fig 6) also contribute to explain the ability of OALC to disrupt preformed biofilm in P. aeruginosa (Fig 5). Similarly, it was recently shown that phenazine binding to extracellular DNA is important for P. aeruginosa biofilm formation (Das et al., 2015) [89]. Indeed, authors demonstrated significant decrease in biofilm formation by the P. aeruginosa ΔphzA-G mutant and enhancement in ΔphzA-G biofilms in the presence of exogenous pyocyanin. Since OALC reduces the production of pyocyanin (one of the phenazines produced by P. aeruginosa; Fig 2), biofilms might also be disrupted by a lack of pyocyanin in the extracellular matrix, thereby weakening the biofilm structure.
Exopolysaccharides are considered as crucial components for biofilm formation and its maintenance in P. aeruginosa. Indeed, most Pseudomonas strains, including PAO1 strain, rely on Psl and Pel polysaccharides for cell-surface, cell-to-cell interactions as well as for adherence to host cells [62] and for biofilm formation [23, 90, 91]. As total extracellular polysaccharides production is reduced upon treatment with OALC (Fig 7), a lower availability in Psl and Pel is reasonably considered. Although we didn’t quantify Psl production, the hypothesis that OALC targets Psl biosynthesis and/or accumulation in biofilm matrix could explain the disruption in biofilm structures observed in one day-old biofilms treated with OALC (Fig 5B). Indeed, Psl functions as a scaffold, holding cells together in the biofilm matrix [90] and the psl operon is also essential for biofilm formation in PAO1 strains, as Psl is involved in both early- and late-stages of biofilm development as well as in the maintenance of biofilm structure so that preformed biofilm can be structurally affected in absence of continuous Psl supply [90, 92]. In contrast, one can assume that the sole inhibition of Pel polysaccharide production could not explain the negative impact in biofilm formation by PAO1 as ΔpelD mutant have been shown to not exhibit significant reduction in biofilm formation compared to PAO1 wild type [93]. As a consequence of polysaccharide defects induced by OALC (Fig 7), biofilm biomass is reduced (Fig 4) and planktonic lifestyle is promoted (Fig 4B) and further experiments are now required to determine if OALC promotes biofilm dispersal, particularly production of c-di-GMP, small regulatory RNAs (RsmY and RsmZ) as well as flagellar motility should be investigated as they are intimately implicated in biofilm dispersion [94].
The negative effect of OALC on las and rhl systems was correlated with a significant reduction in the corresponding concentrations of inducer signals, 3-oxo-C12-HSL and C4-HSL, respectively (Fig 2). However, the reduction of native AHLs is not compensated by exogenous AHLs supply (S6 Fig), indicating that OALC target is beyond AHLs synthesis in the QS pathways. Therefore, we hypothesized that the starting point for the disruption of QS (inhibition of las and rhl systems) and biofilm formation (mainly the reduction in polysaccharides and rhamnolipids production as well as bacterial motility) could be associated with the inhibition of gacA expression by OALC (see Fig 10 for the proposed inhibition cascade). In this model, the two-component regulatory system GacS/GacA that normally inactivate the RNA binding protein, RsmA [95] are presumably impaired at gacA gene level. Consequently, an increase of free RsmA should be observed which lead to the repression of lasI and rhlI gene expression and therefore, the inhibition of bacterial behaviors (including motilities and biofilm formation) and extracellular virulence factors controlled by the las and rhl systems [96, 97]. Likewise, regulations of Pel and Psl production are also presumably disrupted as high levels of free RsmA repress psl and pel expressions and therefore disrupt biofilm formation [98, 99].
[Figure omitted. See PDF.]
Fig 10. Proposed targets and inhibition cascade occurring in P. aeruginosa in presence of OALC.
In P. aeruginosa, OALC inhibits gacA gene expression (key component of GacS/GacA/Rsm signal transduction pathway) leading to an increased level of free RsmA [95]. The latter negatively regulates las and rhl systems leading to inhibition of rhamnolipids, pyocyanin and elastase production [9] as well as components involved in biofilm formation and maintenance, including motilities (swarming and twitching) and Psl/Pel productions [107] independently of QS systems. Exopolysaccharides production is also reduced directly by RsmA [99].
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The in vitro ability of OALC to “weaken” the biofilm matrix as a physical barrier protecting encapsulated bacteria cells against antibiotics is probably at the origin of the observed OALC-tobramycin synergistic activity (Figs 8 and 9). As a result, the antibiotics may better penetrate into the biofilm layers, acting efficiently on bacterial cells more than it could be in structured mature biofilm where antibiotics fail to reach entire bacterial population within the matrix. Our data indicate that this OALC-tobramycin synergistic activity could depend on the observed reduction in polysaccharides production (see Fig 7). Consistently, previous studies have shown that PAO1 biofilm polysaccharides (Pel and Psl, particularly) confer protection against aminoglycoside antibiotics [23] and fast-acting antibiotic defense by affecting the interaction between antibiotics and bacterial cell wall [62, 100]. Thus, synergistic effect of OALC is not linked to an increase of bactericidal activity but rather in an increase of availability of tobramycin inside biofilm matrix. Moreover, several studies corroborate that degraded or at least weakened-biofilm by anti-biofilm compounds through anti-QS or other mechanisms enhance antibiotic action against bacterial biofilms although no mechanism has been clearly proposed by authors [101, 102].
Anti-virulence propriety of OALC was further evidenced by using C. elegans, one of the simplest invertebrate models for studying the P. aeruginosa-host interactions [103]. Previous studies demonstrated that P. aeruginosa PAO1 kills C. elegans but the QS-deficient lasR and lasI rhlI double mutant strains which fail to produce fully AHLs presumably like PAO1 in presence of OALC (Fig 2), appear strongly attenuated in this virulence model [50, 51]. Herein, pre-incubation of PAO1 with OALC considerably reduced the expression of bacterial pathogenic traits, although the treatment was less efficient compared to the reference compound 4-NPO (S7 Fig).
In this study, although the concentration of 200μM is higher than azithromycin (2.67 μM) and is hardly feasible for clinical treatment [69], OALC appears as a potent chemical backbone candidate for further structure-activity studies. OALC is composed of two moieties; an oleanane-type triterpene bearing a p-coumaroyl group. Bodini et al. [104] have demonstrated that p-coumarate exhibits a QSI effect in Chromobacterium violaceum, Agrobacterium tumefaciens and P. putida. Moreover, other studies indicate that oleanolic acid inhibits the in vitro biofilm formation by S. aureus and P. aeruginosa [105, 106]. Accordingly, the dual effect of OALC on both QS regulation and biofilm formation could be linked to the coumaroyl and oleanane groups, respectively. Thus, detailed quantitative structure-activity relationship analysis of the various radicals and cycles as well as the substitutions of the ester link might shed light on the chemical functions required for the anti-QS and anti-biofilm activities of OALC and might lead to more active and stable compounds, with reduced toxicity; an important criteria for drug development.
Supporting Information
[Figure omitted. See PDF.]
S1 Text. Chromatographic fractionation of D. trichocarpa bark extract and isolation of OALC.
Following first fractionation of n-hexane extracts of D. trichocarpa barks (residue of 40 g; see experimental procedures for protocol details), nine fractions were collected from the column chromatography. All of them (except fraction 2) were found to inhibit QS-related (lasB and rhlA) genes expression and/or biofilm formation without affecting bacterial growth (S1A Fig). For further exploration, active fraction products were selected on the basis of the following criteria (i) bacterial growth was not affected; (ii) anti-QS and anti-biofilm formation activities are noticeable; and (iii) amounts of collected residues allowed further fractionation and chemical characterization of the active compound(s). Accordingly, fraction 4 was selected for further fractionation by prep-HLPC to yield the active subfraction F4-5 and F4-7 (S1B Fig). However, only purified compound from subfraction F4-7 (30 mg) was further characterized due to limited quantity of purified compound from subfraction F4-5 (3 mg).
https://doi.org/10.1371/journal.pone.0132791.s001
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S2 Text. Structural elucidation of the active compound as oleanolic aldehyde coumarate.
The active compound was isolated as a white powder and was visualized on TLC plate as a pinkish-purple dark spot following spraying with a vanillin-H2SO4 reagent, suggesting the occurrence of a terpenoid skeleton [108]. The UV spectrum profile (λmax: 203, 226, 308.8 nm) suggested the presence of a 4-oxygenated cinnamic acid derivative [109, 110] (S2A Fig). The ESI-MS (rel. int. %) analysis of active compound revealed a [M−H]− pseudo-molecular peak ion at m/z 585.52 (100), five peaks at m/z 293.06 (10), 621.14 (72), 623.15 (32), 1207.25 (18) and at m/z 1170.98 (30) (S2B Fig). 1H-NMR spectrum showed two obvious groups of signals, one group corresponding to a terpenoid moiety and the other group to a cinnamic acid moeity (S3 Fig). One proton showed singlet at δ 9.40 indicating H-28 in carbonyl carbon; the typical signals for the olefinic double bond H-12 of the structure were obvious from one broad singlet (or t-like) at δ 5.34 (1H) and one proton doublet of doublets at δ 4.61 (J = 8.80, 7.60 Hz), suggesting the presence of H-3. Two doublets (1H each) at δ 6.30 (J = 16.0 Hz) and δ 7.61 (J = 16.0 Hz) are evidence of the presence of trans-coupled protons H-8' and H-7', respectively. Two doublets (2H each) at δ 6.82 (J = 8.4 Hz) and δ 7.43 (J = 8.4 Hz) are assignable to aromatic protons H-3', 5' and H-2', 6', respectively [111, 112]. The 13C NMR spectrum of the active compound also exhibited characteristic signals for one ester carbonyl group at δ 167.4 (S2 Table), four olefinic carbons at δ 123.4 (C-12), δ 143.2 (C-13), 144.3 (C-7’) and δ 116.4 (C-8’), four aromatic signals at δ 116.1 (C-3’, 5’), δ 127.4 (C-1’), δ 130.1 (C-2’, 6’), and δ 158.0 (C-4’), and one hydroxylated carbons at δ 81.0 (C-3). At this stage, by comparison of their physical and spectroscopic data (1H-NMR, 13C-NMR) with those reported in the literature, the above-described characteristics of active compound present some similarity to cinnamoyl triterpenes, such as the p-coumaroyloleanolic acid isolated from Hippophae rhamnoides branch bark and Bauhinia purpurea bark [78, 113] and, more recently, the (3β)-(4-hydroxy-E-cinnamoyl) olean-5,12-dien-28-ol isolated from Crotalaria incana leaves [114]. Finally, unambiguous assignment of the active compound was achieved through 2D NMR [1H-1H correlation spectroscopy (COSY), heteronuclear single quantum coherence (HSQC), heteronuclear multiple bond correlation (HMBC) and nuclear overhauser effect spectroscopy (NOESY)] experiments (S3 Fig). Based on these spectroscopic data, the active compound was identified as a 3β-hydroxyolean-12-en-28-al 3-p-coumarate or oleanolic aldehyde coumarate (OALC, C39H54O4) (Fig 1).
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S1 Table. P. aeruginosa strains and plasmids used in this study.
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S2 Table. 1H- and 13C-NMR spectral data of 3β-hydroxyolean-12-en-28-al 3-p-coumarate (400/400 MHz, CDCl3, δ (ppm) (J = Hz)).
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S3 Table. Construction of plamids pLP170_gacA and pLP170_vfr.
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S1 Fig. Chromatographic scheme of D. trichocarpa bark fractionation steps used to isolate the major QS and biofilm inhibitory compound.
(A) Silica gel column chromatography eluted with hexane/EtOAc gradient mixture (10:0–0:10) and then EtOAc/MeOH (10:0–0:10). Bioactivity was monitored using QS-related (lasB and rhlA) genes expression and biofilm formation; significant inhibition activity was scored “+”. Active fraction 4 was eluted from the column chromatography with the solvent mixture hexane/EtOAc (7:3). (B) High performance liquid chromatogram profile of active fraction F4 monitored at 300 nm. HPLC conditions: injection, 20 μg; column, RP Atlantis dC18 5μm (4.6 by 250 mm); H2O-acetonitrile gradient (10:90 in 5 min, 10:90 to 0:100 in 12 min, 0:100 in 3 min, 0:100 to 10:90 in 2 min, 10:90 in 8 min); 1 mL min-1. Activity was monitored using QS-related gene expression and biofilm formation. Significant inhibition activity was shown for subfraction F4-5 and F4-7.
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S2 Fig. UV and mass spectra of OALC.
(A) UV spectrum of OALC. (B) Electrospray ionization mass spectrum of OALC. Mass spectrum was acquired by direct injection into an electrospray ionization source operated in the negative mode on Finnigan LCQ DUO mass spectrometer. Scans were averaged over 1 min with following conditions: solvent acetonitrile; concentration loaded 10 μg mL-1; negative ionization mode; nebulizer tip set at 250°C and 4.52 kV; cone voltage set at 5 kV; sheath gas (nitrogen) flow rate at 28 arbitrary units; collision energy at -70 eV; MS data were acquired in the m/z range from 50 to 2000.
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S3 Fig. NMR spectrum of OALC.
(A) 1H NMR spectrum of OALC in CDCl3 (400 MHz). (B) 13C NMR spectrum of OALC in CDCl3 (400 MHz). (C) HSQC NMR spectrum of OALC in CDCl3 (400 MHz). (D) HMBC NMR spectrum of OALC in CDCl3 (400 MHz). (E) COSY NMR spectrum of OALC in CDCl3 (400 MHz). (F) NOESY NMR spectrum of OALC in CDCl3 (400 MHz).
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S4 Fig. Effect of OALC at different concentrations (50 to 200 μM) on the expression of PAO1 QS-regulated genes lasB and rhlA and QS independent gene aceA after 18 hours of incubation.
(A) Effect of OALC on QS-regulated lasB gene expression. (B) Effect of OALC on QS-regulated rhlA gene expression. (C) Effect of OALC on QS independent aceA gene expression. The cell density of the bacteria was assessed at 600 nm (clear bar) and gene expression was measured as the β-galactosidase activity of the lacZ gene fusions and expressed in Miller units (grey bar). Naringenin (Nar, 4 mM) is used as a quorum sensing inhibitor control and naringin (Nin, 4 mM) as a negative control. Error bars represent the standard errors of the means and all experiments were performed in quintuplicate with three independent assays and asterisks indicate samples that are significantly different from the DMSO (Student’s t-tests; P ≤ 0.01).
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S5 Fig. Growth kinetics of P. aeruginosa PAO1 in the presence of DMSO 1% or 200 μM OALC.
PAO1 cell viability was assessed after 8h and 18 h by C.F.U. measurement. The statistical significance of each test (n = 5) was evaluated by Student’s t test (i.e. each test was compared with the DMSO condition), and a P value of < 0.01 was considered significant.
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S6 Fig. Effectof OALC on the production of (A) elastase and (B) pyocyanin after exogenous supply of homoserine lactones to wild type strain PAO1. Effect of OALC on the production of (C) elastase and (D) pyocyanin after exogenous supply of the appropriate AHLs to mutant strains, respectively, ΔlasI (ΔPA1432, mutant ID 11174) and ΔrhlI (ΔPA3476, mutant ID 32454).
Productions of pyocyanin and elastase were quantified as in Fig 2. In each case, bacteria were incubated with DMSO, naringenin (Nar), naringin (Nin), OALC, C4-HSL or 3-oxo-C12-HSL). Bacteria were also induced with the appropriate AHL and simultaneously treated with naringenin (+ Nar) or (+Nin) or OALC (+ OALC). C4-HSL and 3-oxo-C12-HSL were added at 10 μM final concentration. DMSO-treated cultures were used as controls, the statistical significance of each test (n = 5) was evaluated by conducting one-way ANOVA with Tukey’s multiple comparison tests, and a P value of ≤ 0.01 was considered significant (asterisks indicate samples that are significantly different from the DMSO). For mutant ΔlasI and ΔrhlI, the letters above the histograms indicate that the data are statistically different from each other (P ≤ 0.01).
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S7 Fig. Mortality of C. elegans nematodes living on a lawn of PAO1 and reduced virulent strains treated with DMSO 1%, naringenin (4 mM), naringin (4 mM) or OALC (200 μM).
(A) Mortality of C. elegans nematodes living on a lawn of P. aeruginosa PAO1 treated with DMSO 1%, naringenin (4 mM), naringin (4 mM) or OALC (200 μM). (B) Mortality of C. elegans nematodes living on a lawn of ΔPA1430 (ΔlasR). (C) Mortality of C. elegans nematodes living on a lawn of ΔPA3477 (ΔrhlR). (D) Toxicity effect of OALC at different concentration (100 μM, 200 μM or 300 μM) and naringenin at 4mM (See experimental procedures for details). Bars show an average of five experiments, and errors bars indicate the standard deviation between experiments. *, data that are statistically different (p ≤ 0.01).
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Acknowledgments
This research was supported by the project PIC-Madagascar 2009 of the ARES-CCD (Académie de Recherche et d’Enseignement Supérieur-Commission Coopération au Développement, Belgium) and by David and Alice Van Buuren foundation, Université Libre de Bruxelles. We would like to thank Professor Barbara Iglewski, Rochester University (School of Medicine and Dentistry), USA, for kindly providing plasmids pPCS223, pPCS1001, pLPR1 and pPCS1002; Professor Junichi Kato, Hiroshima University (Department of Molecular Biotechnology), Japan, for kindly providing plasmids pQF50, pb01, pb02 and pb03; Professor Helmut Görisch, Technische Universität Berlin (Fachgebiet Technische Biochemie, Institut für Biotechnologie), Germany, for providing plasmid pTB4124; Professor David Perez Morga (Centre for Microscopy and Molecular Imaging and Institut de Biologie et de Médecine Moléculaire, Université Libre de Bruxelles, Belgium) for providing access to and helping with the use of the Leica DM IRE2 inverted fluorescence microscope; and University of Minnesota (Minneapolis MN 55455) for providing Caenorhabditis elegans N2 and Escherichia coli OP50 strain. The technical help of Mrs Marie Faes and Mr Olivier Vaillant is gratefully acknowledged.
Author Contributions
Conceived and designed the experiments: MEJ OMV TR AA AR. Performed the experiments: TR OMV CR MK LP JH PD CS. Analyzed the data: PD CS MEJ TR OMV AA AR. Contributed reagents/materials/analysis tools: MEJ PD CS AA AR CR. Wrote the paper: TR OMV PD CS MEJ.
Citation: Rasamiravaka T, Vandeputte OM, Pottier L, Huet J, Rabemanantsoa C, Kiendrebeogo M, et al. (2015) Pseudomonas aeruginosa Biofilm Formation and Persistence, along with the Production of Quorum Sensing-Dependent Virulence Factors, Are Disrupted by a Triterpenoid Coumarate Ester Isolated from Dalbergia trichocarpa, a Tropical Legume. PLoS ONE 10(7): e0132791. https://doi.org/10.1371/journal.pone.0132791
1. Livermore DM (2012) Fourteen years in resistance. Int J Antimicrob Agents 39: 283–294. pmid:22386741
2. WHO (2014) Antimicrobial resistance: global report on surveillance. WHO Press, Geneva Switzerland. 257 pages (ISBN: 978 92 4 156474 8) http://www.who.int/drugresistance/documents/surveillancereport/en
3. Giannakaki V, Miyakis S (2012) Novel antimicrobial agents against multi-drug-resistant gram-positive bacteria: an overview. Recent Pat Antiinfect Drug Discov 7(3):182–188. pmid:23016758
4. Lewis K (2013) Platforms for antibiotic discovery. Nat Rev Drug Discov 12: 371–387. pmid:23629505
5. Kalia VC, Purohit HJ (2011) Quenching the quorum sensing system: potential antibacterial drug targets. Crit Rev Microbiol 37(2): 121–140. pmid:21271798
6. Tay SB, Yew WS (2013) Development of quorum-based anti-virulence therapeutics targeting gram-negative bacterial pathogens. Int J Mol Sci 14(8):16570–16599. pmid:23939429
7. Defoirdt T, Boon N, Bossier P (2010) Can bacteria evolve resistance to quorum sensing disruption? PLoS Pathog 6(7): e1000989. pmid:20628566
8. Rutherford ST, Bassler BL (2012) Bacterial quorum sensing: its role in virulence and possibilities for its control. Cold Spring Harb Perspect Med 2(11): pii: a012427. pmid:23125205
9. Jimenez PN, Koch G, Thompson JA, Xavier KB, Cool RH, Quax WJ (2012) The multiple signaling systems regulating virulence in Pseudomonas aeruginosa. Microbiol Mol Biol Rev 76: 46–65. pmid:22390972
10. Deep A, Chaudhary U, Gupta V (2011) Quorum sensing and bacterial pathogenicity: From molecules to disease. J Lab Physicians 3(1): 4–11. pmid:21701655
11. Williams P, Camara M (2009) Quorum sensing and environmental adaptation in Pseudomonas aeruginosa: a tale of regulatory networks and multifunctional signal molecules. Curr Opin Microbiol 12: 182–191. pmid:19249239
12. Hoge R, Pelzer A, Rosenau F, Wilhelm S (2010) Weapons of a pathogen: proteases and their role in virulence of Pseudomonas aeruginosa. In Current research, technology and education topics in applied microbiology and microbial biotechnology. Méndez-Vilas A. (ed). Badajoz (Spain): Formatex Research Center, pp. 383–395.
13. Reis RS, Pereira AG, Neves BC, Freire DM (2011) Gene regulation of rhamnolipid production in Pseudomonas aeruginosa–a review. Bioresour Technol 102: 6377–6384. pmid:21498076
14. Gupta P, Gupta RK, Harjai K (2013) Multiple virulence factors regulated by quorum sensing may help in establishment and colonisation of urinary tract by Pseudomonas aeruginosa during experimental urinary tract infection. Indian J Med Microbiol 31: 29–33. pmid:23508426
15. Latifi A, Foglino M, Tanaka K, Williams P, Lazdunski AA (1996) hierarchical quorum-sensing cascade in Pseudomonas aeruginosa links the transcriptional activators LasR and RhIR (VsmR) to expression of the stationary-phase sigma factor RpoS. Mol Microbiol 21: 1137–1146. pmid:8898383
16. Medina G, Juarez K, Diaz R, Soberon-Chavez G (2003) Transcriptional regulation of Pseudomonas aeruginosa rhlR, encoding a quorum-sensing regulatory protein. Microbiology 149: 3073–3081. pmid:14600219
17. Wade DS, Calfee MW, Rocha ER, Ling EA, Engstrom E, Coleman JP et al. (2005) Regulation of Pseudomonas quinolone signal synthesis in Pseudomonas aeruginosa. J Bacteriol 187: 4372–4380. pmid:15968046
18. McKnight SL, Iglewski BH, Pesci EC (2000) The Pseudomonas quinolone signal regulates rhl quorum sensing in Pseudomonas aeruginosa. J Bacteriol 182(10): 2702–2708. pmid:10781536
19. Albus AM, Pesci EC, Runyen-Janecky LJ, West SE, Iglewski BH (1997) Vfr controls quorum sensing in Pseudomonas aeruginosa. J Bacteriol 179: 3928–3935. pmid:9190808
20. Reimmann C, Beyeler M, Latifi A, Winteler H, Foglino M, Lazdunski A, Haas D (1997) The global activator GacA of Pseudomonas aeruginosa PAO positively controls the production of the autoinducer N-butyryl-homoserine lactone and the formation of the virulence factors pyocyanin, cyanide, and lipase. Mol Microbiol 24: 309–319. pmid:9159518
21. O’Toole GA (2003) To build a biofilm. J Bacteriol 185: 2687–2689. pmid:12700246
22. Wei Q, Ma LZ (2013) Biofilm matrix and its regulation in Pseudomonas aeruginosa. Int J Mol Sci 14(10): 20983–21005. pmid:24145749
23. Colvin KM, Gordon VD, Murakami K, Borlee BR, Wozniak DJ, Wong GCL et al. (2011) The Pel polysaccharide can serve a structural and protective role in the biofilm matrix of Pseudomonas aeruginosa. PLoS Pathog 7(1): e1001264.
24. Tolker-Nielsen T (2014) Pseudomonas aeruginosa biofilm infections: from molecular biofilm biology to new treatment possibilities. APMIS Suppl 138: 1–51.
25. Byrd MS, Bing P, Wenzhou H, Elizabeth A, Richard A, Chelsie E et al. (2011) Direct Evaluation of Pseudomonas aeruginosa Biofilm Mediators in a Chronic Infection Model. Infect Immun 79(8): 3087–3095. pmid:21646454
26. von Rosenvinge EC, O’May GA, Macfarlane S, Macfarlane GT, Shirtliff ME (2013) Microbial biofilms and gastrointestinal diseases. Pathog Dis 67: 25–38. pmid:23620117
27. Wagner VE, Iglewski BH (2008) Pseudomonas aeruginosa Biofilms in CF Infection. Clinic Rev Allerg Immunol 35: 124–134.
28. Christensen LD, van Gennip M, Jakobsen TH, Alhede M, Hougen HP, Høiby N et al. (2012) Synergistic antibacterial efficacy of early combination treatment with tobramycin and quorum-sensing inhibitors against Pseudomonas aeruginosa in an intraperitoneal foreign-body infection mouse model. J Antimicrob Chemother 67(5): 1198–1206. pmid:22302561
29. LaSarre B, Federle MJ (2013) Exploiting Quorum Sensing To Confuse Bacterial Pathogens. Microbiol Mol Biol Rev 77(1): 73–111. pmid:23471618
30. Rasamiravaka T, Jedrzejowski A, Kiendrebeogo M, Rajaonson S, Randriamampionona D, Rabemanantsoa C et al. (2013) Endemic Malagasy Dalbergia species inhibit quorum sensing in Pseudomonas aeruginosa PAO1. Microbiology 159(5): 924–938.
31. Smith AW, Iglewski BH (1989) Transformation of Pseudomonas aeruginosa by electroporation. Nucleic Acids Res 17:10509. pmid:2513561
32. Jacobs MA, Alwood A, Thaipisuttikul I, Spencer D, Haugen E, Ernst S et al. (2003) Comprehensive transposon mutant library of Pseudomonas aeruginosa. Proc Natl Acad Sci USA 100: 14339–14344. pmid:14617778
33. Vandeputte OM, Kiendrebeogo M, Rasamiravaka T, Stévigny C, Duez P, Rajaonson S et al. (2011) The flavanone naringenin reduces the production of quorum sensing-controlled virulence factors in Pseudomonas aeruginosa PAO1. Microbiology 157(7): 2120–2132.
34. Zhang X, Bremer H (1995) Control of the Escherichia coli rrnB P1 promoter strength by ppGpp. J Biol Chem 270: 11181–11189. pmid:7538113
35. Vandeputte OM, Kiendrebeogo M, Rajaonson S, Diallo B, Mol A, El Jaziri M et al. (2010) Identification of catechin as one of the flavonoids from Combretum albiflorum bark extract that reduces the production of quorum-sensing controlled virulence factors in Pseudomonas aeruginosa PAO1. Appl Environ Microbiol 76: 243–253. pmid:19854927
36. Kretzschmar U, Khodaverdi V, Jeoung JH, Görisch H (2008) Function and transcriptional regulation of the isocitrate lyase in Pseudomonas aeruginosa. Arch Microbiol 190: 151–158. pmid:18574579
37. Pinzon NM, Ju LK (2009) Analysis of rhamnolipid biosurfactants by methylene blue complexation. Appl Microbiol Biotechnol 82(5): 975–981. pmid:19214498
38. Makemson J, Eberhard A, Mathee K (2006) Simple electrospray mass spectrometry detection of acylhomoserine lactones. Luminescence 21: 1–6. pmid:16078303
39. Ishida T, Ikeda T, Takiguchi N, Kuroda A, Ohtake H, Kato J (2007) Inhibition of quorum sensing Pseudomonas aeruginosa by N-acyl cyclopentylamides. Appl Environ Microbiol 73(10): 3183–3188. pmid:17369333
40. Müh U, Schuster M, Heim R, Singh A, Olson ER, Greenberg EP (2006) Novel Pseudomonas aeruginosa quorum-sensing inhibitors identified in an ultra-high-throughput screen. Antimicrob Agents Chemother 50: 3674–3679. pmid:16966394
41. Köhler T, Curty LK, Barja F, Van Delden C, Pecher JC (2000) Swarming of Pseudomonas aeruginosa is dependent on cell-to-cell signaling and requires flagella and pili. J Bacteriol 182: 5990–5996. pmid:11029417
42. Glessner A, Smith RS, Iglewski BH, Robinson JB (1999) Roles of Pseudomonas aeruginosa las and rhl quorum-sensing systems in control of twitching motility. J Bacteriol 181: 1623–1629. pmid:10049396
43. Darzins A (1993) The pilG gene product, required for Pseudomonas aeruginosa pilus production and twitching motility, is homologous to the enteric single-domain response regulator CheY. J Bacteriol 175: 5934–5944. pmid:8104179
44. Khalilzadeh P, Lajoie B, El Hage S, Furiga A, Baziard G, Berge M, Roques C (2010) Growth inhibition of adherent Pseudomonas aeruginosa by an N-butanoyl-L-homoserine lactone analog. Can J Microbiol 56: 317–325. pmid:20453898
45. Jakobsen TH, van Gennip M, Phipps RK, Shanmugham MS, Christensen LD, Alhede M, et al. (2012) Ajoene, a sulphur-rich molecule from garlic, inhibits genes controlled by quorum sensing. Antimicrob Agents Chemother 56: 2314–2325. pmid:22314537
46. Gong AS, Bolster CH, Benavides M, Walker SL (2009) Extraction and Analysis of Extracellular Polymeric Substances: Comparison of Methods and Extracellular Polymeric Substance Levels in Salmonella pullorum SA 1685. Environ Eng Sci 26(10): 1523–1532.
47. Dubois M, Gilles KA, Hamilton JK, Rebers PA, Smith F (1956) Colorimetric method for determination of sugars and related substances. Anal Chem 28(3): 350–356.
48. Torino MI, Taranto MP, Sesma F, de Valdez GF (2001) Heterofermentative pattern and exopolysaccharide production by Lactobacillus helveticus ATCC 15807 in response to environmental pH. J Appl Microbiol 91: 846–852. pmid:11722662
49. Knutson CA, Jeanes A (1968) A new modification of the carbazole analysis: application to heteropolysaccharides. Anal Biochem 24: 470–481. pmid:5723302
50. Rasmussen TB, Bjarnsholt T, Skindersoe ME, Hentzer M, Kristoffersen P, Kote M et al. (2005) Screening for quorum-sensing inhibitors (QSI) by use of a novel genetic system, the QSI Selector. J Bacteriol 187: 1799–1814. pmid:15716452
51. Adonizio A, Leal SM Jr, Ausubel FM, Mathee K (2008) Attenuation of Pseudomonas aeruginosa virulence by medicinal plants in a Caenorhabditis elegans model system. J Med Microbiol 57: 809–813. pmid:18566137
52. Hope IA (1999) C. Elegans: A Practical Approach. New York, USA: Oxford University Press.
53. Gnoula C, Guissou I, Dubois J, Duez P (2007) 5(6)-Carboxyfluorescein diacetate as an indicator of Caenorhabditis elegans viability for the development of an in vitro anthelmintic drug assay. Talanta 71: 1886–1892.
54. Pérez-Martínez I, Haas D (2011) Azithromycin inhibits expression of the GacA-dependent small RNAs RsmY and RsmZ in Pseudomonas aeruginosa. Antimicrob Agents Chemother 55(7): 3399–3405. pmid:21537014
55. Sauer K, Cullen MC, Rickard AH, Zeef LAH, Davies DG, Gilbert P (2004) Characterization of nutrient-induced dispersion in Pseudomonas aeruginosa PAO1 biofilm. J. Bacteriol. 186: 7312–7326. pmid:15489443
56. Klausen M, Heydorn A, Ragas P, Lambertsen L, Aaes-Jørgensen A, Molin S, et al. (2003) Biofilm formation by Pseudomonas aeruginosa wild type, flagella and type IV pili mutants. Mol Microbiol 48(6): 1511–1524. pmid:12791135
57. Klausen M, Aaes-Jørgensen A, Molin S, and Tolker-Nielsen T (2003) Involvement of bacterial migration in the development of complex multicellular structures in Pseudomonas aeruginosa biofilms. Mol Microbiol 50(1): 61–68. pmid:14507363
58. Shrout JD, Chopp DL, Just CL, Hentzer M, Givskov M, Parsek MR (2006) The impact of quorum sensing and swarming motility on Pseudomonas aeruginosa biofilm formation is nutritionally conditional. Mol Microbiol 62: 1264–1277. pmid:17059568
59. Franklin MJ, Nivens DE, Weadge JT, Howell PL (2011) Biosynthesis of the Pseudomonas aeruginosa extracellular polysaccharides, alginate, Pel, and Psl. Front Microbiol Cell Infect Microbiol 167(2): 1–16.
60. Mogayzel PJ Jr, Naureckas ET, Robinson KA, Mueller G, Hadjiliadis D, Hoag JB, et al. (2013) Pulmonary Clinical Practice Guidelines Committee. Cystic fibrosis pulmonary guidelines: chronic medications for maintenance of lung health. Am J Respir Crit Care Med.187:680–689. pmid:23540878
61. Drenkard E (2003) Antimicrobial resistance of Pseudomonas aeruginosa biofilms. Microb. Infect. 5:1213–1219.
62. Yang L, Hu Y, Liu Y, Zhang J, Ulstrup J, Molin S (2011) Distinct roles of extracellular polymeric substances in Pseudomonas aeruginosa biofilm development. Environ Microbiol 13(7): 1705–1717. pmid:21605307
63. Tseng BS, Zhang W, Harrison JJ, Quach TP, Song JL, Penterman J. et al. (2013) The extracellular matrix protects Pseudomonas aeruginosa biofilms by limiting the penetration of tobramycin. Environ Microbiol 15: 2865–2878.
64. Gallagher LA, Manoil C (2001) Pseudomonas aeruginosa PAO1 kills Caenorhabditis elegans by cyanide poisoning. J Bacteriol 183: 6207–6214.
65. Darby C, Cosma CL, Thomas JH, Manoil C (1999) Lethal paralysis of Caenorhabditis elegans by Pseudomonas aeruginosa. Proc Natl Acad Sci USA 96: 15202–15207. pmid:10611362
66. Reardon S (2014) WHO warns against “post-antibiotic” era. Agency recommends global system to monitor spread of resistant microbes. Nature news (30 April 2014) http://www.nature.com/news/who-warns-against-post-antibiotic-era-1.15135.
67. Blackledge MS, Worthington RJ, Melander C (2013) Biologically inspired strategies for combating bacterial biofilms. Curr Opin Pharmacol 13(5): 699–706. pmid:23871261
68. Rasamiravaka T, Labtani Q, Duez P, El Jaziri M (2015) The Formation of Biofilms by Pseudomonas aeruginosa: A Review of the Natural and Synthetic Compounds Interfering with Control Mechanisms. BMRI 2015: Article ID 759348.
69. Imperi F, Leoni L, Visca P (2014) Antivirulence activity of azithromycin in Pseudomonas aeruginosa. Front Microbiol 5:178. pmid:24795709
70. Kim H-S, Lee S-H, Byun Y, Park H-D (2015) 6-Gingerol reduces Pseudomonas aeruginosa biofilm formation and virulence via quorum sensing inhibition. Sci Rep 5 (8656)
71. Zhou L, Zheng H, Tang Y, Yu W, Gong Q (2013) Eugenol inhibits quorum sensing at sub-inhibitory concentrations. Biotechnol Lett 35(4): 631–637.
72. Cady NC, McKean KA, Behnke J, Kubec R, Mosier AP, Kasper SH et al. (2012) Inhibition of biofilm formation, quorum sensing and infection in Pseudomonas aeruginosa by natural products-inspired organosulfur compounds. PLoS One 7(6): e38492. pmid:22715388
73. Lemmens RHMJ (2008) Dalbergia trichocarpa Baker. [Internet] Fiche de Protabase. Louppe D., Oteng-Amoako A.A., Brink M. (Editeurs). PROTA (Plant Resources of Tropical Africa / Ressources végétales de l’Afrique tropicale), Wageningen, The Netherlands. http://database.prota.org/recherche.htm.
74. Narayanan MC, Rao PR, Shanmugam NN, Gopalakrishnan SM, Devi K (2007) Isolation and characterisation of bioactive isoflavonoids from the roots of Dalbergia horrida. Nat Prod Res 21(10): 903–909. pmid:17680501
75. Songsiang U, Wanich S, Pitchuanchom S, Netsopa S, Uanporn K, Yenjai C (2009) Bioactive constituents from the stems of Dalbergia parviflora. Fitoterapia 80(7): 427–431. pmid:19524648
76. Rajaonson S, Vandeputte OM, Vereecke D, Kiendrebeogo M, Ralambofetra E, Stévigny C et al. (2011) Virulence quenching with a prenylated isoflavanone renders the Malagasy legume Dalbergia pervillei resistant to Rhodococcus fascians. Environ Microbiol 13: 1236–1252. pmid:21332623
77. Ravindranath N, Ravinder Reddy M, Ramesh C, Ramu R, Prabhakar A, Jagadeesh B, et al. (2004) New lathyrane and podocarpane diterpenoids from Jatropha curcas. Chem Pharm Bull 52: 608–611. pmid:15133216
78. Yang ZG, Li HR, Wang LY, Li YH, Lu SG, Wen XF et al. (2007) Triterpenoids from Hippophae rhamnoides L. and their nitric oxide production inhibitory and DPPH radical-scavenging activities. Chem Pharm Bull 55(1): 15–18. pmid:17202693
79. Tanachatchairatana T, Bremner JB, Chokchaisiri R, Suksamrarn A (2008) Antimycobacterial activity of cinnamate-based esters of the triterpenes betulinic, oleanolic and ursolic acids. Chem Pharm Bull 56(2): 194–198. pmid:18239308
80. Hu JF, Garo E, Goering MG, Pasmore M, Yoo HD, Esser T et al. (2006) Bacterial biofilm inhibitors from Diospyros dendo. J Nat Prod 69(1): 118–120. pmid:16441080
81. de Kievit TR (2009) Quorum sensing in Pseudomonas aeruginosa biofilms. Environ Microbiol 11(2): 279–288. pmid:19196266
82. Li YH, Tian X (2012) Quorum Sensing and Bacterial Social Interactions in Biofilms. Sensors 12: 2519–2538. pmid:22736963
83. Hentzer M, Riedel K, Rasmussen TB, Heydorn A, Andersen JB, Parsek MR et al. (2002) Inhibition of quorum sensing in Pseudomonas aeruginosa biofilm bacteria by a halogenated furanone compound. Microbiology 148(1): 87–102.
84. Pamp SJ, Tolker-Nielsen T (2007) Multiple roles of biosurfactants in structural biofilm development by Pseudomonas aeruginosa. J Bacteriol 189: 2531–2539. pmid:17220224
85. Patriquin G, Banin E, Gilmour C, Tuchman R, Greenberg EP, Poole K (2008) Influence of quorum-sensing and iron on twitching motility and biofilm formation in Pseudomonas aeruginosa. J Bacteriol 190: 662–671. pmid:17993517
86. O’Toole GA, Kolter R (1998) Flagellar and twitching motility are necessary for Pseudomonas aeruginosa biofilm development. Mol Microbiol 30(2): 295–304. pmid:9791175
87. Davey ME, Caiazza NC, O’Toole GA (2003) Rhamnolipid surfactant production affects biofilm architecture in Pseudomonas aeruginosa PAO1. J Bacteriol 185: 1027–1036. pmid:12533479
88. Nickzad A, Déziel E (2014) The involvement of rhamnolipids in microbial cell adhesion and biofilm development—an approach for control? Lett Appl Microbiol 58(5): 447–453. pmid:24372465
89. Das T, Kutty SK, Tavallaie R, Ibugo AI, Panchompoo J, Sehar S, et al. (2015) Phenazine virulence factor binding to extracellular DNA is important for Pseudomonas aeruginosa biofilm formation. Sci Rep 5 (8398)
90. Ma L, Jackson KD, Landry RM, Parsek MR, Wozniak DJ (2006) Analysis of Pseudomonas aeruginosa conditional Psl variants reveals roles for the Psl polysaccharide in adhesion and maintaining biofilm structure postattachment. J Bacteriol 188: 8213–8221. pmid:16980452
91. Ma L, Conover M, Lu H, Parsek MR, Bayles K, Wozniak DJ (2009) Assembly and development of the Pseudomonas aeruginosa biofilm matrix. PLoS Pathog 5: e1000354. pmid:19325879
92. Jackson KD, Starkey M, Kremer S, Parsek MR, Wozniak DJ (2004) Identification of psl, a locus encoding a potential exopolysaccharide that is essential for Pseudomonas aeruginosa PAO1 biofilm formation. J Bacteriol 186: 4466–4475. pmid:15231778
93. An S, Wu J, Zhang L-H (2010) Modulation of Pseudomonas aeruginosa biofilm dispersal by a cyclic-Di-GMP phosphodiesterase with a putative hypoxia-sensing domain Appl Environ Microbiol 76(24): 8160–8173. pmid:20971871
94. Chua SL, Liu Y, Yam JKH, Chen Y, Vejborg RM, Tan S et al. (2014) Dispersed cells represent a distinct stage in the transition from bacterial biofilm to planktonic lifestyles. Nat Commun 5. 4462. pmid:25042103
95. Brencic A, McFarland KA, McManus HR, Castang S, Mogno I, Dove SL et al. (2009) The GacS/GacA signal transduction system of Pseudomonas aeruginosa acts exclusively through its control over the transcription of the RsmY and RsmZ regulatory small RNAs. Mol Microbiol 73(3): 434–445. pmid:19602144
96. Pessi G, Williams F, Hindle Z, Heurlier K, Holden MT, Camara M, et al. (2001) The global posttranscriptional regulator RsmA modulates production of virulence determinants and N-acylhomoserine lactones in Pseudomonas aeruginosa. J Bacteriol 183: 6676–6683.
97. Kay E, Humair B, Denervaud V, Riedel K, Spahr S, Eberl L et al. (2006) Two GacA dependent small RNAs modulate the quorum-sensing response in Pseudomonas aeruginosa. J Bacteriol 188(16): 6026–6033. pmid:16885472
98. Ventre I, Goodman AL, Vallet-Gely I, Vasseur P, Soscia C, Molin S et al. (2006) Multiple sensors control reciprocal expression of Pseudomonas aeruginosa regulatory RNA and virulence genes. Proc Natl Acad Sci USA 103:171–176. pmid:16373506
99. Irie Y, Starkey M, Edwards AN, Wozniak DJ, Romeo T, Parsek MR (2010) Pseudomonas aeruginosa biofilm matrix polysaccharide Psl is regulated transcriptionally by RpoS and post-transcriptionally by RsmA. Mol Microbiol 78(1):158–172. pmid:20735777
100. Billings N, Millan MR, Caldara M, Rusconi R, Tarasova Y, Stocker R et al. (2013) The Extracellular Matrix Component Psl Provides Fast- Acting Antibiotic Defense in Pseudomonas aeruginosa Biofilms. PLoS Pathog 9(8): e1003526. pmid:23950711
101. Busetti A, Shaw G, Megaw J, Gorman SP, Maggs CA, Gilmore BF (2014) Marine-derived quorum-sensing inhibitory activities enhance the antibacterial efficacy of tobramycin against Pseudomonas aeruginosa. Mar Drugs 13(1): 1–28. pmid:25546516
102. Moreau-Marquis S, Coutermarsh B, Stanton BA (2015) Combination of hypothiocyanite and lactoferrin (ALX-109) enhances the ability of tobramycin and aztreonam to eliminate Pseudomonas aeruginosa biofilms growing on cystic fibrosis airway epithelial cells. J Antimicrob Chemother 70(1): 160–166. pmid:25213272
103. Papaioannou E, Utari PD, Quax WJ (2013) Choosing an Appropriate Infection Model to Study Quorum Sensing Inhibition in Pseudomonas Infections. Int J Mol Sci 14(9): 19309–19340. pmid:24065108
104. Bodini SF, Manfredini S, Epp M, Valentini S, Santori F (2009) Quorum sensing inhibition activity of garlic extract and p-coumaric acid. Lett Appl Microbiol 49: 551–555. pmid:19709367
105. Wolska KL, Grudniak AM, Fiecek B, Kraczkiewicz-Dowjat A, Kurek A (2010) Antibacterial activity of oleanolic and ursolic acids and their derivatives. Cent Eur J Biol 5: 543–553.
106. Kiplimo JJ, Koorbanally NA, Chenia HY (2011) Triterpenoids from Vernonia auriculifera Hiern exhibit antimicrobial activity. Afr J Pharm Pharmacol 5: 1150–1156.
107. Sakuragi Y, Kolter R (2007) Quorum-sensing regulation of the biofilm matrix genes (pel) of Pseudomonas aeruginosa. J Bacteriol 189: 5383–5386. pmid:17496081
108. Jermain JD, Evans HK (2009) Analyzing salvia divinorum and its active ingredient salvinorin a utilizing thin layer chromatography and gas chromatography/mass spectrometry. J Forensic Sci 54(3): 612–616. pmid:19298461
109. Määttä KR, Kamal-Eldin A, Törrönen AR (2003) High-performance liquid chromatography (HPLC) analysis of phenolic compounds in berries with diode array and electrospray ionization mass spectrometric (MS) detection: Ribes species. J Agric Food Chem 51: 6736–6744. pmid:14582969
110. Stalikas CD (2007) Extraction, separation, and detection methods for phenolic acids and flavonoids. J Sep Sci 30: 3268–3295. pmid:18069740
111. Kuo YH, Chang CI, Kuo YH (1997) Triterpenes from Diospyros maritime. Phytochemistry 46: 1135–1137.
112. Takahashi H, Iuchi M, Fujita Y, Minami H, Fukuyama Y (1999) Coumaroyl triterpenes from Casuarina equisetifolia. Phytochemistry 51: 543–550.
113. Kuo Y-H, Chu P-H (2002) Studies on the Constituents from the Bark of Bauhinia purpurea. J Chin Chem Soc 49: 269–274.
114. Zafrul Azam ATM, Moni F, Hamiduzzaman Md, Mehedi Masud M, Mahmood Hasan C (2013) Two Cinnamoyl Triterpenes and Steroids from Crotalaria incana (Fabaceae). Res J Phytochem 7: 1–9.
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Abstract
Recently, extracts of Dalbergia trichocarpa bark have been shown to disrupt P. aeruginosa PAO1 quorum sensing (QS) mechanisms, which are key regulators of virulence factor expression and implicated in biofilm formation. One of the active compounds has been isolated and identified as oleanolic aldehyde coumarate (OALC), a novel bioactive compound that inhibits the formation of P. aeruginosa PAO1 biofilm and its maintenance as well as the expression of the las and rhl QS systems. Consequently, the production of QS-controlled virulence factors including, rhamnolipids, pyocyanin, elastase and extracellular polysaccharides as well as twitching and swarming motilities is reduced. Native acylhomoserine lactones (AHLs) production is inhibited by OALC but exogenous supply of AHLs does not restore the production of virulence factors by OALC-treated cultures, indicating that OALC exerts its effect beyond AHLs synthesis in the QS pathways. Further experiments provided a significant inhibition of the global virulence factor activator gacA by OALC. OALC disorganizes established biofilm structure and improves the bactericidal activity of tobramycin against biofilm-encapsulated PAO1 cells. Finally, a significant reduction of Caenorhabditis elegans paralysis was recorded when the worms were infected with OALC-pre-treated P. aeruginosa. Taken together, these results show that triterpenoid coumarate esters are suitable chemical backbones to target P. aeruginosa virulence mechanisms.
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