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The Gram negative anaerobe Fusobacterium nucleatum has been implicated in the aetiology of periodontal diseases. Although frequently isolated from healthy dental plaque, its numbers and proportion increase in plaque associated with disease. One of the significant physico-chemical changes in the diseased gingival sulcus is increased environmental pH. When grown under controlled conditions in our laboratory, F. nucleatum subspecies polymorphum formed mono-culture biofilms when cultured at pH 8.2. Biofilm formation is a survival strategy for bacteria, often associated with altered physiology and increased virulence. A proteomic approach was used to understand the phenotypic changes in F. nucleatum cells associated with alkaline induced biofilms. The proteomic based identification of significantly altered proteins was verified where possible using additional methods including quantitative real-time PCR (qRT-PCR), enzyme assay, acidic end-product analysis, intracellular polyglucose assay and Western blotting.
Of 421 proteins detected on two-dimensional electrophoresis gels, spot densities of 54 proteins varied significantly (p<0.05) in F. nucleatum cultured at pH 8.2 compared to growth at pH 7.4. Proteins that were differentially produced in biofilm cells were associated with the functional classes; metabolic enzymes, transport, stress response and hypothetical proteins. Our results suggest that biofilm cells were more metabolically efficient than planktonic cells as changes to amino acid and glucose metabolism generated additional energy needed for survival in a sub-optimal environment. The intracellular concentration of stress response proteins including heat shock protein GroEL and recombinational protein RecA increased markedly in the alkaline environment. A significant finding was the increased abundance of an adhesin, Fusobacterial outer membrane protein A (FomA). This surface protein is known for its capacity to bind to a vast number of bacterial species and human epithelial cells and its increased abundance was associated with biofilm formation.
This investigation identified a number of proteins that were significantly altered by F. nucleatum in response to alkaline conditions similar to those reported in diseased periodontal pockets. The results provide insight into the adaptive mechanisms used by F. nucleatum biofilms in response to pH increase in the host environment.
Bacteria in nature are exposed to changing environmental conditions; they sense and detect signals from their surroundings and gene expression is regulated in response to specific cues in harsh environments to adapt and survive . The anaerobic Gram negative oral bacterium, Fusobacterium nucleatum, is frequently isolated from both supra- and sub-gingival dental plaque in humans and has been implicated in the aetiology of periodontal disease [2-4]. This bacterium is one of the most common oral species isolated from human extra-oral infections and abscesses including blood, brain, liver, abdomen and genital tract . Increasing evidence also suggests that F. nucleatum is associated with an increased risk of preterm birth [5-8] while two latest studies indicated a possible association between the presence of F. nucleatum and bowel tumors [9,10].
Studies have reported that the pH of the periodontal pocket in humans suffering from periodontitis is alkaline and may be as high as 8.9 [11-13]. It is also reported that localised pH gradients ranging between 3 and 8 occur within a 10-species oral biofilm model . The alkalinity in the disease state is largely due to the release of ammonium ions produced from the catabolism of amino acids and peptides derived from gingival crevicular fluid (GCF) by proteolytic bacteria [15,16]. Previous studies in our laboratory showed that when grown in a chemostat between pH 6 and 8, F. nucleatum grew as planktonic culture . We have also reported that increasing the culture pH to 8.2 induced biofilm growth and the cells exhibited significant increases in length and surface hydrophobicity . This pH alkaline-induced phenotypic switch to biofilm growth observed may be an adaptive mechanism in response to adverse environmental pH that occurs during the progression of periodontal disease in vivo. This bacterium has been demonstrated to survive in calcium hydroxide treated root canal systems at pH 9.0  and in a separate study, biofilm growth conferred protection to root canal bacteria at pH 10 . Biofilm formation by F. nucleatum may provide protection to cells when exposed to alkaline environments. Bacteria growing in biofilms exhibit altered phenotypes and are more resistant to antimicrobial agents and the host immune system . The characterisation of biofilms has revealed that cells within them exhibit different concentrations in proteins involved in metabolism, transport and regulation [22-25]. Protein regulation in F. nucleatum in response to acidic (pH 6.4) and mild alkaline (pH 7.4 and 7.8) has been reported [26,27].
The present study uses a proteomic approach to examine changes in protein expression by F. nucleatum associated with biofilm formation induced by growth at pH 8.2. Where possible, the expression of proteins that was significantly altered was validated using enzyme assay, acidic end-product analysis, Western blotting and qRT-PCR. This study identified 54 proteins with significantly altered concentrations in alkaline-induced F. nucleatum biofilms that may reflect changes in cellular functions that occur in the diseased environment.
F. nucleatum subsp. polymorphum (ATCC 10953) was purchased from Cryosite (NSW, Australia) and maintained on anaerobic blood agar plates (Thermo Fischer, Vic, Australia). The bacterium was cultured anaerobically using a model C-30 Bio-Flo Chemostat (New Brunswick Scientific, NJ, USA) as previously described, with minor modifications . Briefly, a chemically defined growth medium based on that of van der Hoeven  was supplemented with 10mM glucose, 20mM glutamic acid, 10mM histidine and 10mM lysine (all other amino acids were 1mM). Amino acids were purchased from Sigma Aldrich (St Louis, MO, USA). During planktonic growth, the medium was pumped at a flow rate of 27mL/h to give an imposed dilution rate of D=0.069/h. Using the relationship, Tg (generation time)=ln 2/D, this gave a bacterial generation time of 10h. Such generation time of the culture mimics the growth rate of bacteria in mature dental plaque (generation time between 7–12h) . Initially, the culture was maintained at pH 7.4±0.1 which was optimal for growth of the organism at 37°C . The planktonic culture was harvested after steady state was achieved (10 generations). The culture was removed from the culture vessel and stored at −80°C until use. The growth pH was then increased by 0.2 unit increments to 8.2±0.1 over an 8h period. Several hours after pH 8.2 was achieved, F. nucleatum cells adhered to surfaces of the culture vessel and formed biofilms. Biofilm cells were harvested by increasing culture agitation during sampling to dislodge adherent cells. Cell aggregates from detached biofilms were allowed to settle for 2min. Planktonic cells were carefully decanted and the remaining biofilm cells were used for further analyses. Bacterial cultures grown under both pH conditions were harvested daily, for five consecutive days, and pooled as biological replicates.
Bacterial cells were collected by centrifugation (8,000×g, 4°C, 10min) and lysed by sonication (Soniprobe, Dawe Instruments, England; 1.8 A for 5cycles, 10s each) on ice. Unbroken cells were removed by centrifugation at 2,500×g (4°C, 10min). Centrifugation of cell free lysates at 20,000×g (4°C, 30min) was performed to pellet the cell envelope (inner and outer membranes). Cytoplasmic proteins present in the supernatant were prepared as described previously  and membrane proteins were prepared from the cell envelope fraction using the method described by Molloy and colleagues  with slight modifications.
Briefly, precipitation of cytoplasmic proteins was performed by incubating samples with ice cold acetone (four sample volumes) containing 50mM dithiothreitol (DTT; Sigma Aldrich, St Louis, MO, USA) overnight at −20°C. Protein precipitate was collected by centrifugation at 10,000×g (2°C, 30min). Membrane proteins were extracted by resuspending cell pellets in sodium carbonate (0.1M, pH 11) and stirred on ice for 1h. The carbonate-treated membranes were collected by ultra-centrifugation (115,000×g, 4°C, 1h). Extracted cytoplasmic and membrane proteins were then solubilised with ReadyPrep Reagent 3 (Bio-Rad Laboratories, CA, USA) containing 5M urea, 2M thiourea, 2% (w/v) CHAPS, 2% (w/v) detergent sulfobetaine 3–10, 40mM Tris, 0.2% Bio-lyte 3/10 and 2mM tributyl phosphine and stored at −80°C until required.
Protein quantification was performed using Reducing Agent and Detergent Compatible Protein Assay Kit (Bio-Rad Laboratories, CA, USA) prior to 2DE. Gel-based isoelectric focusing (IEF) was performed using a PROTEAN IEF Cell (Bio-Rad Laboratories, CA, USA) using pre-cast Immobilised pH Gradient (IPG) strips with an isoelectric point (pI) range of 4–7 or 7–10 and proteins were cup-loaded onto the anode end of IPG strips. Optimal protein load and IEF running conditions are listed in Additional file 1: Table S1. Cytoplasmic proteins with a pI between 7 and 10 required an additional liquid-based IEF separation prior to 2DE. A total of 10mg of solubilised cytoplasmic proteins were separated into 10 fractions between pI 3 and 10 using a MicroRotofor Liquid-Phase IEF Cell (Bio-Rad Laboratories, CA, USA). Liquid-based IEF was performed at 20°C at 1W for 2h. The fractions between pI 7 and 10 were pooled and following protein determination, separated by 2DE.
Following 2DE IEF, IPG strips were incubated in 2% (w/v) DTT in equilibration buffer (6M urea, 2% (w/v) SDS, 0.05M Tris/HCl buffer (pH 8.8) and 20% (v/v) glycerol), followed by 2.5% (w/v) iodoacetamide in equilibration buffer for 15min each. Proteins were then separated on 20×20cm polyacrylamide (12%T, 3.3% C, 0.1% SDS, 375mM Tris/HCl, pH 8.8) gels using a PROTEAN II XL Multi-Cell (Bio-Rad Laboratories, CA, USA) which allowed six gels to be run simultaneously. Gels were stained with either Coomassie Brilliant Blue R-250 (Sigma Aldrich, MO, USA) or Flamingo Fluorescent Stain (Bio-Rad Laboratories, CA, USA) and scanned using a GS-800 Densitometer (Bio-Rad Laboratories, CA, USA) or Typhoon Scanner (GE Healthcare, Buckinghamshire, UK), respectively.
Image analysis of the 2-DE gels was performed using PD-Quest 7.2 Software (Bio-Rad Laboratories, CA, USA). Six gels were produced for each pI range (4–7 and 7–10) for cytoplasmic and cell membrane proteins from either biofilm or planktonic cells (48 gels in total). Replicate groups containing four to six highly reproducible gels from either planktonic or biofilm cells were used for analysis. Spot intensities were normalised using the total density in gels. Spot detection was performed using the automated spot detection algorithm before being checked and matched manually. Matchsets containing gel images were created to identify proteins that showed significant changes in concentration (at least two-fold changes in spot intensities at a significance level of p <0.05, Student’s t-test). Analysis sets comparing growth conditions containing proteins that appeared in all replicate gels which showed significant quantitative changes were identified and proteins were excised from gels for MS analysis and protein identification.
All mass spectrometry (MS) instruments and analysis software were purchased from Bruker Daltonics GmbH (Bremen, Germany). The excised protein spots were digested with trypsin, destained and digested as described before .
One microlitre of each sample was applied to a 600μm AnchorChip according to the α-cyano-4-hydroxycinnamic acid method . MALDI-TOF mass spectra were acquired using a Bruker Ultraflex III MALDI-TOF/TOF mass spectrometer operating in reflectron mode under the control of the flexControl software (Version 3.0). Peptide standards were used to perform external calibration under identical conditions. MS spectra were collected randomly across each AnchorChip spot. Optimal laser intensity and shot count were both operator determined. Those spectra which exhibited high signal to noise MS peaks were summed together to generate a final peptide MS fingerprint spectrum. Between three and six of the most highly abundant sample ions (i.e. non-trypsin and non-keratin) were selected as precursors for MS/MS analysis. MALDI-TOF/TOF was performed in the LIFT mode using the same spot on the target . MS and MS/MS spectra were subjected to smoothing, background subtraction and peak detection using flexAnalysis (version 3.0). The spectra and mass lists were exported to BioTools (version 3.1). The MS and corresponding MS/MS spectra were combined and submitted to the in-house Mascot database-searching engine (version 2.2, Matrix Science: http://www.matrixscience.com) using the following specifications:
Database: NCBI non-redundant 20080622, 20081114 and 20100216
Fixed modifications: carbamidomethyl (C)
Variable modifications: oxidation (M)
Mass tol MS: 50 p.p.m
MS/MS tol: 0.5Da
Missed cleavages: 1
Protein identification was based upon the MOWSE and probability scored generated by the software. Based on the combined MS/Ms data, samples that returned a positive ‘hit’ were submitted independently to Mascot.
Samples that failed to give sufficient spectra using MALDI MS/MS for accurate protein identification were further analysed using LC-ESI ion trap MS/MS. Peptides were separated by chromatography using an Agilent Protein ID Chip column assembly (40nL trap column with 0.075×43mm C-18 analytical column) housed in an Agilent HPLC-Chip Cube Interface (Agilent Technologies, CA, USA) connected to an a HCT ultra 3D-Ion-Trap mass spectrometer. The column was equilibrated with 4% acetonitrile containing 0.1% formic acid at 0.5 μL min-1 and the samples eluted with an acetonitrile gradient (4%-31% in 32min). MS/MS spectra of ionisable species were acquired in a data-dependant fashion as follows: Ionisable species (300<m/z<1200) were trapped and the two most intense ions in the scan were independently fragmented by collision-induced dissociation. Post acquisition, MS and MS/MS spectra were subjected to peak detection using Bruker’s DataAnalysis software (version 3.4). Data were imported into BioTools. MS/MS data were searched as described above, but with an MS mass tolerance and MS/MS tol of 0.3 and 0.4Da, respectively, and a peptide charge of 1+, 2+ and 3+.
The intracellular concentrations of heat shock protein (HSP) GroEL and a recombination protein RecA were analysed by Western blotting. Aliquots of cell lysates from both planktonic and biofilm cultures equivalent to 15μg of protein, were separated by electrophoresis on 12%T 3.3% C polyacrylamide gels (100V, 1.5h) . The proteins were then electro-transferred to an Immuno-Blot PVDF membrane (Bio-Rad Laboratories, CA, USA) using Mini Trans-Blot Cell (250mA, 2h) (Bio-Rad Laboratories, CA, USA) followed by blocking (1h, room temperature) using 5% (w/v) ECL Blocking Agent (GE Healthcare, Buckinghamshire, UK). The washed membrane was then treated with either mouse anti-human Hsp60 monoclonal antibody (SPA-087, Stressgen Biotechnologies, British Columbia, Canada) diluted 1:1000 or mouse anti-E. coli RecA monoclonal antibody (MD-02+3, MBL International, IF, USA) diluted 1:1000 for 24h at 4°C. The washed membrane was then probed for 1h at room temperature with anti-mouse alkaline phosphatase conjugate secondary antibody (1 mAB: 5000 BSA- tris-buffered saline-tween 20 (TBS-T)). The target protein was detected using ECF substrate and scanned using a Typhoon Scanner. The expression of the protein was analysed using ImageQuant TL software. EFC substrate, Typhoon Scanner and ImageQuant TL software were purchased from GE Healthcare (Buckinghamshire, UK).
Gene sequences of groEL, dnaK and recA and 16S rRNA were retrieved from the Oralgen Databases (http://www.oralgen.lanl.gov) and primers were designed using the web-based tool Primer 3-PCR (Additional file 2: Table S2). 16S rRNA was used as reference gene.
Bacterial samples from each culture type (4mL) were harvested and incubated in 4mL of RNAlater (Ambion, Austin, TX, USA) overnight at 4°C. RNAlater was then removed by centrifugation (5,000×g, 4°C, 15min). Cell pellets were resuspended in 1mL of fresh RNAlater and stored at −80°C until required. Total RNA was extracted from the bacterial pellets using the RiboPure-Bacteria Kit (Ambion, TX, USA) following the manufacturer’s instructions. Bacterial cDNA templates were generated from 1μg RNA by reverse transcription using a SuperScript® Vilo™ cDNA Synthesis Kit (Invitrogen, CA, USA). qRT-PCR was performed using a Corbett Rotor-Gene RG-3000 Thermal Cycler (Qiagen, Hilden, Germany) using a standard curve method. Each PCR run consisted of a standard curve and five biological replicate samples for each growth pH. All standards and samples were performed in triplicate. The total reaction volume of 20 μL consisted of 2 μL of each forward and reverse primer, 10 μL of Platinum SYBR Green qPCR SuperMix-UDG (Taq DNA polymerase, SYBR Green I dye, Tris–HCl, KCl, 6mM MgCl2, 400μM dGTP, 400μM dCTP, 800μM dUT, UGG and stabilizers; Invitrogen, CA, USA), 5 μL dH2O and 1 μL of diluted cDNA. The conditions for amplification cycles were as follows: 40cycles consisting of denaturation at 95°C for 15s, annealing at 60°C for 60s, and extension at 72°C for 30s.
Planktonic and biofilm cells were harvested and lysed as described above. A protein assay was performed using Coomassie Plus Protein Assay Kit (Thermo Scientific, Rockford, IL, USA) on each lysate and an equal amount of cell protein was used to measure GDH activity based on the protocol proposed by Irwin and co-workers  with slight modifications. The amount of enzyme in samples was determined by measuring the rate of conversion of NAD+ to NADH over 5min, a reaction that generates a proportional increase in absorbance at 340nm and was measured spectrophotometrically (Lambda 5 Spectrophotometer, Perkin Elmers, Bodenseewerk, Germany). Reaction mixtures contained 1mM NAD+, 4mML-glutamate, 50mM sodium pyrophosphate buffer (pH 8.8) and 50 μL of cell lysate. GDH activity in cell lysates was expressed in GDH unit per mg of cell protein. GDH from bovine liver (Sigma Aldrich, MO, USA) was used to construct a standard curve.
The genome of F. nucleatum subsp. polymorphum (ATCC 1953) codes for 2067 open reading frames (ORFs) . In this study, we examined proteins that are within pI range 4–10, and molecular weight (MW) range 10 and 80kDa, which represents approximately 80% of the F. nucleatum genome . Previous studies resolved whole cell- or cytoplasmic-protein subsets within a 4–8 pI range [26,37-39]. We have also reported the expression of cell envelope proteins in F. nucleatum (pI 4–10) grown at pH 7.8 . In comparison, the present study examined both cytoplasmic and cell membrane protein expression (pI range 4–10) following growth at pH 8.2. As proteins with basic pIs are considered to be difficult to resolve on 2DE gels , optimisation of 2DE conditions was performed to yield satisfactory protein resolution (Additional file 1: Table S1 and Figure Figure1).1). Without MicroRotofor-IEF separation, only a small number of cytoplasmic proteins between pI 7 and 10 were resolved on 2DE gels that contained excessive vertical streaking (data not shown). This was likely due to the comparatively high abundance of soluble proteins in the pI 4–7 range in samples. Prior to 2DE, therefore, proteins with a pI<7 were removed. Protein assay of pooled fractions confirmed that the ratio of acidic (pI 4–7) to basic (pI 7–10) proteins was approximately 4:1 (data not shown). The overcrowding of acidic proteins (pI 4–7) has been reported in microbial species including the parasitic protozoa Leishenia amazonensis. In this study, a reduced amount (100μl) of sample containing enriched cytoplasmic proteins (pI 7–10) was loaded onto 11cm IPG strips. Due to the reduced protein load, gels were stained with Flamingo Fluorescent stain (Additional file 1: Table S1). As only 30% of the bacterial genome encodes for membrane proteins, we also included the separation of cell envelope and cytoplasmic proteins prior to 2DE to improve the detection of membrane proteins .
A total of 31 gels were used for expression analysis. 421 proteins, representing 330 cytoplasmic and 91 membrane proteins, with a pI between 4 and 10 and a MW between 10 and 80kDa were separated and visualised using Coomassie/Flamingo Fluorescent stains (Additional file 1: Table S1). Comparison of 2DE gels representing growth at pH 7.4 and 8.2 revealed that the intracellular concentrations of 54 proteins were significantly (p<0.05) altered at least two-fold (Table (Table1).1). The abundance of 23 proteins either increased marked or exclusively detected in biofilm cells while 31 proteins either decreased in biofilm cells or were only detected in planktonic cells. A number of proteins were identified as potential isoforms arising from post-translational modifications indicated by altered pI and/or MW. Table Table11 summarises proteins identified and groups them according to their functional classes.
Earlier studies in our laboratory showed that the regulation of proteins associated with energy production, transport and protein folding occurred in planktonic cells cultured at pH 7.8 [26,27]. While the present study reports a similar change in protein expression patterns at pH 8.2, we have identified 32 proteins that are altered in response to growth at pH 8.2. It is likely that these proteins may be associated with the altered morphology and biofilm formation observed at the higher pH.
Our data show that metabolic enzyme production was closely associated with a change to biofilm growth at pH 8.2. 31% (17 proteins) of all identified proteins were associated with metabolism and 30% (16 proteins) were substrate-transporters (Table (Table11 and Figure Figure2).2). F. nucleatum is able to catabolise both sugars and amino acids as energy sources [17,19,43], in contrast to the periodontal pathogens Porphyromonas gingivalis and Treponema denticola. Histidine and glutamic acid are among the amino acids that are readily metabolised by F. nucleatum to generate energy and produce ammonia, acetate and butanoate as end-products [45-47]. The bacterium also ferments sugars (glucose, galactose and fructose) to produce a mixture of acetate, formate and lactate .
In the present study, key enzymes involved in the catabolism of glutamate and histidine via the 2-oxoglutarate pathway and pyruvate were significantly altered in biofilm cells (Table (Table1).1). A previous study of F. nucleatum cultured at pH 6.4, 7.4 and 7.8 also revealed the regulation of metabolic enzymes . In contrast to this finding, we found that no glycolytic enzyme concentrations were altered in biofilm cells grown at pH 8.2 compared to planktonic cells grown at 7.4. However, a three-fold increase in glucose utilisation and IP was observed (Table (Table2,2, Figure Figure3).3). It is possible that the observed increase in glucose storage may play an important role in the organism’s survival during periods of nutrient limitation when exposed to pH 8.2 [43,49,50]. Although the expression of glycolytic enzymes was not significantly altered, an increase in lactate dehydrogenase (LDH) (EC 126.96.36.199) and a three-fold increase in lactate production was observed, indicating a metabolic shift at pH 8.2 towards ATP generation via anaerobic glycolysis (Embden-Meyerhof-Parnas pathway) (Tables1 and and2,2, Figure Figure3).3). In addition, at pH 8.2, an increase in acidic end products per mg cellular protein and shift to lactate production was observed (Table (Table2).2). These changes may assist in maintenance of intracellular pH due to the lower pKa of lactic acid (3.08) compared to formic (3.75), acetic (4.75) and butanoic (4.82) acids. .
The proteomic results show that the concentration of six GDH isoforms was significantly altered, two isoforms showed increased concentration while four showed decreased concentration in biofilm cells (Spots 5–10, Figure Figure1;1; Table Table1).1). Total GDH activity was investigated using enzyme assay. Biofilm cells showed a 1.5-fold increase in GDH activity compared to planktonic cells (Table (Table2).2). This finding and their reduced MW suggests that GDH isoforms (Spots 7–10, Table Table1)1) likely represent truncated and inactive forms of the enzyme. A markedly increased (>3-fold) production of GDH compared to pH 7.4 was observed at pH 8.2 (Spots 5 and 6, Table Table1).1). Previous proteomic results showed that when cultured at pH 7.8, F. nucleatum increased the production of GDH by 1.3-fold . This enzyme catalyses the initial oxidation of glutamate in the 2-oxoglutarate pathway (Figure (Figure3)3) and increased abundance of this enzyme would allow the organism to respond metabolically to elevated glutamate levels associated with the increased GCF flow observed in periodontal disease . An increased capacity to catabolise glutamate at an elevated environmental pH may give the organism a selective advantage. Interestingly, previous studies reported differing observations with an increased intracellular concentration of GDH in an aero-tolerant strain of F. nucleatum subsp. nucleatum but not in bacterial cells cultured under oxidative stress .
At pH 7.4, butanoate was the dominant amino acid metabolite produced by F. nucleatum (Table (Table2).2). This appears associated with the increased intracellular concentration of butanoate: acetoacetate CoA transferase (EC 188.8.131.52) and a decreased concentration of butyryl-CoA dehydrogenase (EC 184.108.40.206) in planktonic compared to biofilm cells (Table (Table1,1, Figure Figure3).3). Growth at pH 8.2 revealed an increased acetate/butanoate ratio (Table (Table2).2). This finding was consistent with the observed decreased expression of butyryl-CoA dehydrogenase (EC 220.127.116.11) and butanoate: acetoacetate CoA transferase (EC 18.104.22.168) and increased production of phosphate acetyltransferase (EC 22.214.171.124) in biofilm cells (Table (Table1,1, Figure Figure3).3). A shift from butanoate to acetate production by F. nucleatum under oxidative stress was also reported by Steeves and colleagues . The production of the more oxidized end-product (acetate) yields more biomass per mole than butanoate . Accordingly, it has been suggested that this shift towards acetate is energy efficient, yielding more ATP per mole of crotonoyl-CoA . A decreased production of pyruvate synthase (EC 126.96.36.199) was observed in cells cultured at pH 8.2 (Table (Table1).1). This enzyme catalyses the inter-conversion of pyruvate to acetyl-CoA, linking the 2-oxoglutarate and glycolytic pathways. The decreased intracellular concentration of this enzyme potentially uncouples the two pathways in the biofilm cells (Figure (Figure33).
Approximately 10% of bacterial genes encode for transport proteins, the majority of these are located in bacterial membranes . The expression of bacterial membrane genes and proteins, particularly outer membrane proteins, is of great interest as they are directly involved in the cell’s interaction with the environment and perform essential roles in bacterial adaptation to host niches .
Bacterial transport proteins are classified according to their mechanism and include primary active transporters, secondary transporters, channels and pores . In the present study, the intracellular concentration of 16 transport-associated proteins (five porins and 11 substrate-specific transporters) was significantly altered by a pH increase to 8.2 (Table (Table1).1). The increased intracellular concentration of TRAP transporters and increased concentration of ABC transporter binding proteins could be considered to be energy conserving as TRAP transporters rely on proton-motive force instead of ATP hydrolysis (ABC transporters) to drive the uptake of solutes from the environment. In contrast to our results, the production of TRAP transporter binding proteins was suppressed 10-fold in planktonic cells cultured at pH 7.8 . The authors explained that the decreased abundance of TRAP binding proteins in planktonic cells may be due to a reduced proton gradient . However, bacterial cells growing within a biofilm structure may be more protected from pH fluctuation and the loss of protons to the environment. This may explain the increased production of TRAP transporters in biofilms was observed.
The virulence of F. nucleatum is largely due to the adhesive properties that allow the bacterium to interact with perio-dontopathogens and host cells during the onset of periodontal disease. Two identified adhesins, RadD and FomA, are among the outer membrane proteins that are responsible for interspecies and host cell interactions [58-60]. The intracellular concentration of the adhesin FomA did not appear to be altered by planktonic F. nucleatum cells when cultured at pH 7.8 . In the present study, however, the abundance levels of four FomA isoforms, with isoelectric points varying between 7 and 9, increased significantly in biofilm cells (Table (Table1).1). A preliminary study in the laboratory indicated that two FomA isoforms (spots 41 and 42, Figure Figure11 and Table Table1)1) could be phosphorylated (data not shown) and further studies are required to determine the roles of these isofoms in biofilm cells. The protein is thought to be associated with mature plaque biofilm development as it facilitates the coaggregation between F. nucleatum and other bacteria such as P. gingivalis[60,61]. A more recent study demonstrated that in a mouse periodontitis model a bacterial suspension of P. gingivalis and F. nucleatum neutralised with anti-FomA antibody showed a significant reduction in abscess formation and gingival swelling . Our results support the suggestion that FomA is a potential vaccine target for periodontal disease.
As mentioned previously, significant changes in cell morphology were associated with F. nucleatum biofilm formation . Biofilm cells cultured at pH 8.2 presented with a significant increase in length. This altered morphology may be associated with a decrease in production of the RND superfamily antiporters (Table (Table1).1). Although better known as a multidrug-exporter, this protein also plays a role in bacterial cell division . A member of the RND superfamily, EnvC protein, has been reported to be responsible for septum formation in Escherichia coli.
In this study, the intracellular concentrations of HSPs 70kDa chaperone protein DnaK, 60kDa chaperonin GroEL and peptidyl-prolyl cis-trans isomerase (PPI), and a recombination protein, RecA, were influenced by environmental pH (Table (Table1).1). Growth at pH 8.2 resulted in elevated levels of both GroEL and PPI and decrease levels of DnaK. Although constitutive, their production is influenced by stress conditions . The regulation of DnaK, GroEL and PPI in response to environmental pH was also observed in previous studies [26,27]. Compared to pH 7.4, it appears that the concentration of both GroEL and PPI increase significantly at both pH 7.8 and 8.2. Our proteomic results indicate that the intracellular concentration of DnaK decreased at least 4-fold in biofilm cells (Table (Table1).1). This protein plays a role in nascent polypeptide folding and may reflect decreased growth rate and protein synthesis associated with culture at pH 8.2.Western blotting and qRT-PCR were performed to confirm the proteomic results (Figure (Figure4).4). It was not possible to validate the abundance of DnaK protein using Western blotting as F. nucleatum DnaK failed to cross react with the mouse anti-E. coli DnaK monoclonal antibody used (data not shown). qRT-PCR, however, supported the proteomic results by showing a 2.9-fold decrease in expression (p<0.01) of dnaK at pH 8.2 (Figure (Figure4c).4c). Western blotting revealed a 1.4-fold increase in GroEL (Figure (Figure4a)4a) while qRT-PCR gave a contrasting result indicating significantly decreased groEL expression (3-fold) in biofilm cells. Contrasting results were also observed in the transcript and protein levels of recA and its product. The proteomic data demonstrated at least 10-fold increase of RecA in biofilm cells while qRT-PCR results showed a significant 1.8-fold down-regulation of recA in biofilm cells (Figure (Figure4;4; Table Table11).
The chaperonin GroEL has been suggested to function at later stages of protein folding and is required for post-translational folding of unfolded or partially folded peptides  and protein degradation [66,67]. The increased intracellular concentration of this stress protein at pH 8.2 may prevent protein aggregation and misfolding due to an increased intracellular pH. Bacterial GroEL is highly homologous with human HSP 60. It was shown to cross-react with human HSP 60 on endothelial cells and induces autoimmune responses that may play a role in the process of vascular endothelial injury, a key event in the pathogenesis of atherosclerosis . A recent study by Lee and colleagues  reported that F. nucleatum GroEL induces a number of risk factors in a mouse model of atheroscleorosis. The increased production of GroEL under alkaline pH environments may support the association between periodontal diseases and atherosclerosis.
The intracellular concentration of RecA, which is associated with the maintenance and repair of DNA, was found to increase at pH 8.2 (Table (Table1).1). Both acidic (<pH 5.0) and alkaline (>pH 8.0) pH environments denature DNA via depurination leading to the separation of double-stranded DNA [70,71]. Repair of the DNA gap relies on recombinational DNA proteins, including RecA . The increased production of RecA may reflect the rise in intracellular pH at pH 8.2. Interestingly, our Western blotting results did not detect altered concentration of RecA in cells grown at pH 7.4 and 8.2. The production of RecA under different growth pH may therefore require further investigation although some may argue that Western blotting technique is of semi-quantitative in nature .
The intracellular concentration of seven proteins classified in the category of protein synthesis including five elongation factors (EF-Tu and EF-Ts) and two ribosomal S2 subunits decreased significantly by at least ten-fold at pH 8.2 (Table (Table1).1). Bacterial elongation factors EF-Tu and EF-Ts interact with each other and are essential for growth in E. coli. These proteins are often reported to be differentially expressed by bacterial cells exposed to stressful environments. It is interesting to note that the abundance of elongation factors EF-Ts decreased 2-fold in F. nucleatum when exposed to pH 7.8  but remained affected when the bacterium was cultured under oxidative stress . Elongation factor EF-Tu has been reported to posses chaperone-like properties . Len and co-workers  reported an increased production of EF-Tu at low pH by acid-stressed Streptococcus mutans. The down-regulation of EF-Tu and translational proteins in the present study may indicate reduced rate of protein synthesis at pH 8.2.
To our knowledge, this is the first study to investigate alterations in both cytoplasmic and membrane protein production in F. nucleatum alkaline induced biofilms. Our results indicate that the biofilm cells may be more metabolically efficient, primarily via alterations in glucose and glutamate catabolism. The regulation of membrane transport proteins may assist in energy conservation. In addition, the capacity to remain functional in the suboptimal pH environment may also be attributed to the altered concentration of stress proteins. The significant increased abundance of adhesin FomA at pH 8.2 may be associated with the surface change that promotes biofilm formation. The elongation observed in bacterial cells cultured at pH 8.2 may be due to a decrease abundance of RND transporters that play a role in cells. The altered intracellular concentration three hypothetical proteins reported may be important for coping with pH stress but their roles are yet to be fully investigated. Significant changes in protein concentration were validated using a variety of techniques and generally indicated the high reliability of proteomic data. The shift to biofilm growth and the changed protein expression reflected mechanisms that likely enable F. nucleatum to adapt successfully and compete in its natural habitat in the oral cavity. It has been suggested that interactions between oral bacteria present in dental plaque result in many new physiological functions which cannot be observed in an individual component system . Kuboniwa and colleagues (2009) examined the protein expression of P. gingivalis growing in a three-species system containing the pioneer plaque species Streptococcus gordonii and F. nucleatum revealing the protective mechanisms that may exist within multi-species communities . The development of multi-species biofilm systems in the future may be used to increase knowledge of the gene and protein expression of F. nucleatum.
2DE: Two dimensional electrophoresis; GDH: Glutamate dehydrogenase; GCF: Gingival crevicular fluid; IEF: Isoelectric focusing; pI: Isoelectric point; MW: Molecular weight; PPI: Peptidyl-prolyl cis-trans isomerase; ABC: ATP binding casstte; TRAP: Tripartite ATP-indpendent periplasmic; RND: Resistance-nodulation-cell division; FomA: Fusobacterial outer membrane protein A.
JC conducted all hands-on experimental work and drafted the manuscript. PSZ proposed the study and provided advice on the proteomic investigation. NJG participated in the design of the experiments and provided advice on the enzyme assays and HPLC analysis. JMF provided advice and expertise from a dentist’s perspective and revised the manuscript. All authors read and approved the final manuscript.
Table S1. Summary of 2DE conditions used for separation of cytoplasmic and membrane proteins.
Table S2. Designed primers used for qRT-PCR.
This work was supported by The Australian Dental Research Foundation. J. Chew was supported by Adelaide Scholarships International. We thank Tracy Fitzsimmons, Krzysztof Mrozik, Victor Marino and staff at The Adelaide Proteomics Centre for excellent technical assistance.