Open access peer-reviewed chapter

Biofilm Formation of Salmonella

Written By

Daxin Peng

Submitted: 23 October 2015 Reviewed: 07 March 2016 Published: 13 July 2016

DOI: 10.5772/62905

From the Edited Volume

Microbial Biofilms - Importance and Applications

Edited by Dharumadurai Dhanasekaran and Nooruddin Thajuddin

Chapter metrics overview

3,472 Chapter Downloads

View Full Metrics

Abstract

Salmonella spp. may form biofilm, and bacteria in biofilm are more resistant to drug, chemical, physical and mechanical stresses, and host immune system. The progress on biofilm research will be helpful for the development of new tools and strategies to prevent biofilm-related disease and decontaminate biofilm-derived Salmonella in food production. In this review, we present a comprehensive overview of biofilm formation in Salmonella, included that (1) the component of Salmonella biofilm, (2) the detection methods for biofilm, (3) the identification of biofilm-formation-associated genes, (4) the regulation mechanism of biofilm formation, and (5) virulence or resistance of Salmonella in biofilm.

Keywords

  • Salmonella
  • biofilm
  • component
  • mechanism
  • gene
  • pathogenicity
  • drug resistance

1. Introduction

Salmonella enteric is an intracellular gram-negative pathogen that infects various hosts, which is classified into more than 2500 serovars [1]. Many serovars, such as those most commonly associated with human infections, including Salmonella enteritidis, Salmonella typhimurium, have a broad host range [2]. In contrast, other serovars, such as Salmonella typhi, Salmonella paratyphi, Salmonella gallinarum, Salmonella choleraesuis, Salmonella abortusovis, and Salmonella dublin, have restricted host ranges and are associated primarily with one or a few hosts [3]. Salmonella can cause disease in domestic animals, ranging in severity of asymptom, diarrhea and enteritis to systemic syndrome, and result in a huge economic loss in pig and poultry industry. Salmonellosis is also a growing public health concern in both the developed and developing countries, since nontyphoidal Salmonella disease, a major cause of diarrheal disease globally, is estimated to cause 93 million enteric infections and 155,000 diarrheal deaths each year [4]. The illnesses and outbreaks are most commonly attributed to exposure to contaminated food, and the eggs, broiler chickens, and pigs are among the top sources [5]. Salmonella often exist not only as planktonic cells but also as sessile, multicellular forms such as biofilms attached to surfaces. Biofilm formation is important for the spread of Salmonella because bacteria in the biofilm are resistant to disinfectants and chemical, physical, and mechanical stresses [68]. The biofilm formation is also contributed to Salmonella virulence, since bacteria in the biofilm are more resistant to antibiotics and host immune system, resulting in a chronic infection and the development of Salmonella carrier state [9, 10]. In our review, we present a comprehensive overview of biofilm formation in Salmonella.

Advertisement

2. The component of Salmonella biofilm

The biofilm formation is a multistep developmental process that always has several distinguishable steps: (a) attachment to the carrier surface, reversible, (b) irreversible attachment, binding to the surface with the participation of adhesions or exopolysaccharides, (c) the development of microcolonies, a distinct mushroom shape, (d) the maturation of biofilm architecture [11, 12], (e) under favorable conditions, the synthesis of martrix compounds decreases and the matrix is enzymatically cleaved, leading to biofilm dispersion [13]. In natural environments, Salmonella forms biofilms on plant [14], abiotic surfaces, including plastics, metal and glass [1517], meat and meat-processing environments [18, 19]. In addition, Salmonella can colonize gallstones under laboratory conditions [20], and the Salmonella biofilm can be directly visualized by confocal micrographs of extracellular matrix on the surface of human cholesterol gallstones [21]. They can also form biofilms on chicken intestinal epithelium [22] or HEp-2 cells that are suspended in once-flow-through continuous culture conditions [23].

The extracellular matrix of Salmonella biofilm is majorly composed of curli (amyloid fimbriae), cellulose [24, 25], biofilm-associated protein (Bap) [26], O-antigen capsule [14, 27], extracellular DNA [28, 29]. The expression pattern of the biofilm is serovar specific and correlates with contact surface [30]. Curli were first discovered in the late 1980s on Escherichia coli strains that caused bovine mastitis, and they are mainly involved in adhesion to surfaces, cell aggregation and biofilm formation. Curli also mediate host cell adhesion and invasion, and they are potent inducers of the host inflammatory response [12]. The curli protein is encoded by the divergently transcribed csgBAC (agfBAC) and csgDEFG (agfDEFG) operons [31, 32]. The csgBAC operon encodes the major structural subunit, CsgA, and the surface-exposed nucleator protein CsgB. A third gene, csgC, is in the csgBAC operon, but no transcript for csgC has been detected in curli biogenesis [32]. The other study shows that both CsgC and CsgE facilitate extracellular thin aggregative fimbriae synthesis in Salmonella enteritidis [33]. The csgDEFG operon encodes accessory proteins required for curli assembly. The csgD gene encodes a transcriptional regulator belonging to the LuxR family, CsgD, for active transcription of csgBAC promoter [24]. Although Giaouris et al. [34] found that CsgF was expressed in biofilm growth when compared with planktonic and biofilm cells of Salmonella enteritidis on stainless steel surface, the function of csgF and csgG genes has not been resolved in Salmonella. Cellulose is a polysaccharide composed of β(1 → 4)-linked D-glucose units [35], which is an important exopolysaccharide normally synthesized in the Salmonella biofilms. The production of cellulose and curli by Salmonella leads to a matrix of tightly packed cells covered in a hydrophobic network. The operons, bcsABZD and bcsEFG, are required for cellulose biosynthesis [36]. Cellulose biosynthesis is positively regulated by CsgD, which stimulates the transcription of AdrA that harbours a cytoplasmic GGDEF domain. AdrA activates cellulose production on the post-transcriptional level either by direct interaction with bcs operons or indirect interaction with bis-3′-5′-cyclic dimeric guanosine monophosphate (c-di-GMP) [25, 37, 38]. BapA, a large cell-surface protein required for biofilm formation, is encoded by bapA gene and secreted through a type-I protein secretion system (bapBCD operons) situated downstream of the bapA gene. The expression of bapA is coordinated with that of genes encoding curli fimbriae and cellulose, through the action of csgD [26, 39]. The bapA gene is also highly conserved in Salmonella [40]. Salmonella produces an O-antigen capsule coregulated with the fimbria- and cellulose-associated extracellular matrix. The operons yihU-yshA and yihVW are responsible for capsule assembly and translocation [41] and regulated by CsgD. Although the O-antigen capsule do not appear to be important for multicellular behavior, they play an important role in attachment and environmental persistence [14]. However, the O-antigen capsule is required for biofilm formation of Salmonella typhimurium and Salmonella Typhi on cholesterol gallstones, and the operons are regulated in a csgD-independent manner [42]. Extracellular DNA is shown to be a matrix component of Salmonella biofilms cultivated in flow chambers and on glass surfaces [28]. However, the presence of extracellular DNA plays an inhibitive and destabilizing effect during biofilm development of Salmonella on abiotic surfaces [29].

Advertisement

3. The detection methods for biofilm

3.1. Quantification of biofilm formation

Biofilm formation of Salmonella can be quantitated by microplate-based crystal violet staining [43]. Briefly, the overnight broth cultures of bacterium are diluted 1:100 in the diluted tryptic soy broth (TSB). One hundred µl of bacterial suspension is added into 96-well U-bottomed polystyrene microtiter plates. Plates are incubated at 28°C for 24 h under static conditions. Then, non-adherent bacteria are removed and the wells are washed gently three times with 200 µl of distilled water. One hundred μl of 0.4% crystal violet (v/v) is added into each well and stained for 20 min. After discard of staining liquid, all loosely adhering bacteria and dye are gently washed off with distilled water for three times. The dye bound to the adherent cells is solubilized with 100 µl of anhydrous ethanol per well. The optical density (OD) is measured at 590 nm, and OD value of biofilm-formation strain is significantly higher than that of negative control. It provides more reproducible results with an addition of a fixtion step (80°C for 30 min) prior crystal violet staining [19]. Combined with resazurin assay, the number of metabolically active cells is able to be evaluated [44]. With wheat germ agglutinin-Alexa Fluor 488 conjugate, which selectively binds to N-acetylglucosamine residues in biofilms, the spectrofluorometric assay provides a more sensitive method for quantification and characterization of bacterial biofilms [45].

3.2. Biofilm formation in glass tube

The overnight cultures of bacteria are diluted 1:100 in the diluted TSB. Two milliliters of each bacterial suspension are added into borosilicate glass tubes and incubated at 28°C for 48 h. Then, the liquid is decanted and the tubes are washed gently three times with distilled water. Two ml of 0.4% crystal violet (v/v) are added into each tube and stained at room temperature for 20 min. The stained biofilm is observed at the liquid–air interface on the glass test tube walls or at the bottom of the tube [46]. The glass tubes may also be incubated at 37°C at 200 rpm by using an orbital shaker, and biofilm is observed at interphase without staining [47].

3.3. Congo red/carbol fuchsin staining

The overnight culture (1:100 diluted in TSB) is inoculated into 3 ml of fresh TSB in a 6-well plate containing sterile polystyrene coverslip (20 × 20 mm). After incubation at 28°C for 24 or 48 h without agitation, the coverslips are removed carefully, treated with cetylpyridinium chloride (10 mM) for 30 s, rinsed with distilled water and air dried for 20–30 min. After fixation by gentle heating, the coverslips are stained with a mixture of saturated aqueous Congo red solution and 10% Tween-80 (2:1, V/V) for 30 min and rinsed with distilled water. After staining with 10% (v/v) Ziehl carbol fuchsin for 6 min and rinsing in distilled water, the coverslips are air dried and mounted on slides [48]. Under a light microscope, bacterial cells on slides show purple staining, while the exopolysaccharides of biofilm show pink staining [46].

3.4. Field emission scanning electron microscopy

The coverslips with cultured bacteria are fixed in 3% glutaraldehyde in 0.1 M phosphate-buffered saline at 4°C for 2 h. The samples are then dehydrated with increasing concentrations of ethanol (50, 70, 80, 90, and 100%) followed by isoamyl acetate (100%), each for 15 min. The samples are critical point dried for 5 h, coated with gold palladium alloy, and observed under a field emission scanning electron microscope [49]. The biofilm-formation strain exhibits increased clusters of bacteria cells with curli fimbriae and has meshwork-like structures surrounding the cell surfaces.

3.5. Congo red and calcofluor plates

LB agar plate without salt supplemented with 40 mg/L Congo red and 20 mg/L brilliant blue is used to determine the Congo red-binding property of the colonies. LB agar plate supplemented with 200 mg/L calcofluor (fluorescent brightener) is used to determine the cellulose production by comparing the fluorescence of the test strains under UV light [49]. Biofilm of Salmonella is mainly composed of curli and cellulose, and Salmonella strains were grouped into distinct morphotypes according to Congo red binding: (a) red, dry, and rough indicating curli and cellulose production (RDAR), (b) brown, dry, and rough, indicating a lack of cellulose synthesis (BDAR), (c) pink, dry, and rough, indicating a defect in curli expression (PDAR), (d) smooth, brown, and mucoid, indicating a lack of cellulose synthesis but overproduced capsular polysaccharide (SBAM), and (e) smooth and white, indicating a lack of both curli and cellulose production (SAW) [19, 31, 50].

3.6. Confocal laser microscopy

Bacteria cultured on coverslipes, dish, or microplate are stained by 0.1 M phosphate-buffered saline (pH 7.2) containing SYTO 9 and propidium iodide. After 10 min incubation in the dark at room temperature, stained samples are examined using a confocal scanning laser microscopy. Fluorochromes are excited using an argon laser source at 488 nm. Images are collected in two channels, 490–515 and 620–640 nm, corresponding to the emission maxima for SYTO 9 and propidium iodide, respectively. Optical sections approximately 1 μm in height are collected starting from below the focal plane to upward through the entire biofilm. The biofilm cells are clearly observed in a multilayer community [20, 51].

Advertisement

4. Identification of biofilm-formation–associated genes

The most common biofilm-formation–associated genes are the genes encode adhesins. The best characterized of the Salmonella fimbriae is type-1 fimbriae. This fimbrial type is encoded by the fim gene cluster and is assembled by the chaperone–usher system [52]. The fimA gene encodes the major structural subunit, while the fimH gene encodes the adhesin protein that is located at the tip of the assembled fimbrial structure and mediates binding to the receptor. The FimH adhesin is involved in biofilm formation on HEp-2 tissue culture cells, murine intestinal epithelium, and chicken intestinal epithelium [22, 23]. The long polar fimbriae (Lpf) are encoded by the lpfABCDE genes and have been implicated in the colonization of the murine intestinal mucosa [53, 54]. Plasmid-encoded fimbriae (Pef) are encoded on the 90-kb Salmonella virulence plasmid and are majorly encoded by pefBCD, orf5, and orf6 genes. Both Lpf and Pef contribute to the early steps of biofilm formation [55]. Salmonella enteritidis produce a variety of potentially adherent fimbrial types including SEF14 (SefA), SEF17 (CsgA), SEF18 (SefD), and SEF21 (type I, FimA), the role of each fimbrial in biofilm formation is different. The SEF17 encoded by csgA gene stabilize cell–cell interactions during biofilm formation, while SEF21 fimbriae may involve cell surface adherence [56]. SadA is trimeric autotransporter adhesin of Salmonella typhimurium, the expression of SadA resulted in cell aggregation, biofilm formation, and increased adhesion to human intestinal Caco-2 epithelial cells [57]. Salmonella may persist on post-harvest lettuce during cold storage, the genes stfC, bcsA, misL, and yidR, encoding a fimbrial outer membrane usher, a cellulose synthase catalytic subunit, an adhesin of the autotransporter family expressed from the Salmonella pathogenicity island-3, and a putative ATP-/GTP-binding protein, respectively, have a role in persistence of the pathogen. The bcsA, misL, and yidR knockout mutants are impaired in attachment and biofilm formation, suggesting that these functions are required for biofilm formation [58].

Salmonella flagella are not required for the formation of the multicellular morphotype on plates. However, the global behavior of the bacterial community on air–liquid, surface–liquid, or cell–liquid interfaces is changed in the absence of flagella. In a mutant lacking flagella and thin aggregative fimbriae, the contribution of the latter to the multicellular morphotype is dominant [59]. Biofilm formation of an flgK mutant in meat and poultry broths and their attachment on surfaces of stainless steel and glass are significantly reduced compared with that of the wild-type strain, suggest that expression of flagella could be involved in biofilm formation and attachment of Salmonella on contact surfaces [60]. The presence of the flagellar filament enhances binding and biofilm formation in the presence of bile, while flagellar motility and expression of type-1 fimbriae were unimportant in biofilm formation on cholesterol gallstones [61].

Pathogenicity islands accommodate large clusters of genes that contribute to a particular virulence phenotype. Salmonella possess at least seven salmonella pathogenicity islands (SPIs). Among these, SPI1 is primarily required for bacterial motility and invasion of host cells. Salmonella typhimurium cultures containing cloned SPI-1 display an adherent biofilm and cell clumps in the media. This phenotype was associated with hyper-expression of SPI-1 type-III secretion functions. Surprisingly, mutations in genes essential for known bacterial biofilm pathways (bcsA, csgBA, bapA) did not affect the biofilms formation, indicating that this phenomenon is independent of established biofilm mechanisms [62]. Salmonella biofilm cells exposed to superheated steam show decreased transcription of flagella and SPI-1 genes, respectively, whereas increased transcription of SPI-2 genes, important for bacterial survival and replication inside host cells, is detected [63]. In contrast, when compared biofilms of Salmonella typhimurium with planktonic cells, the most highly downregulated genes in the biofilm are located on SPI-2 and that a functional SPI2 secretion system regulator (ssrA) is required for Salmonella typhimurium biofilm formation. Genes involved in tryptophan (trp) biosynthesis and transport are upregulated in the biofilm. Deletion of trpE results in decreased bacterial attachment and biofilm formation, indicating that aromatic amino acids make an important contribution to biofilm formation [64]. The aro mutants of Salmonella are frequently used as live vaccines for the oral vaccination of domestic animals, and they are unable to synthesize chorismate, which is a key intermediate in the synthesis of aromatic amino acids. The aro mutants exhibit a decreased production of cellulose, N-acetyl-D-glucosamine, or N-acetylneuraminic acid-containing capsular polysaccharide and fimbriae, which explains their inability to form biofilms [65].

Lipopolysaccharide (LPS) synthesis also involves the biofilm formation of Salmonella. Two Tn5 insertion mutations in genes that are involved in ddhC and waaG result in diminished expression of colony rugosity. Both mutants have impaired biofilm formation when grown in rich medium with low osmolarity, they constitutively form larger amounts of biofilms when the growth medium was supplemented with either glucose or a combination of glucose and NaCl [49]. The rfbA gene also involve in lipopolysaccharide biosynthesis. Biofilm formation by the rfbA mutant in meat and poultry broths and their attachment on surfaces of stainless steel and glass is significantly reduced [60]. Using transposon mutagenesis, the genes metE, ompR, rpoS, rfaG, rfaJ, rfaK, rfaP, rfbH, rhlE, spiA, and steB are found to be associated with biofilm formation of Salmonella enteritidis [66, 67]. When eight mutants with knockout of genes ompR, rpoS, rfaG, rfbH, rhlE, metE, spiA, or steB from the Salmonella pullorum are constructed. Only the ompR mutant showed a complete loss of production of curli and biofilm formation. The other mutants showed a modified production of curli and cellulose with less effect related to biofilm formation [68]. Therefore, an integral LPS, at both the O-antigen and core polysaccharide levels, are important in the modulation of curli protein and cellulose production, as well as in biofilm formation.

Advertisement

5. Regulation mechanism of biofilm formation

Biofilm formation is majorly regulated by CsgD protein, a regulator belonging to the LuxR family [69]. CsgD has an N-terminal receiver domain with a conserved aspartate (D59) as a putative target site for phosphorylation and a C-terminal LuxR-like helix-turn-helix DNA binding motif. The unphosphorylated CsgD directly binds the csgBA and adrA promoter regions to activate transcription [70]. Multiple factors bind to the promoter sequence of csgD and regulate its transcription, such as OmpR, RpoS, RpoE, integration host factor (IHF), histone-like nucleoid structuring protein (H-NS), and MlrA. OmpR is one of first discovered to be required for csgD transcription [71]. Six binding sites (D1–D6) for OmpR are identified in csgD promoter regions. Binding of OmpR-P to D2 centered immediately upstream of D1 is proposed to repress promoter activity. IHF competes with OmpR-P for binding at its upstream site IHF1, which overlaps with D3–D6 and thereby activate the transcription of csgD [72]. The mutant of ompR in Salmonella enteritidis and Salmonella pullorum has inability to produce cellulose, curli, and biofilm [68, 73]. RpoS, encodes an alternative sigma factor of RNA polymerase, is critical for bacterial endurance under the most-stressful conditions, including stationary-phase entrance and host adaptation. RpoS is required for transcriptional activation of the csgD promoter in Salmonella typhimurium strains that rdar morphotype are normally expressed at low temperature [31]. However, in two Salmonella typhimurium strains, spontaneous mutants are found forming rdar colonies independent of temperature, the regulation of csgD is independent of rpoS [71]. Partially independent of rpoS for regulation of csgD is observed in Salmonella enteritidis. The rpoS mutant in Salmonella pullorum also shows similar biofilm forming ability as the wild-type strain [68], suggests that another sigma factor may recognize the csgD promoter. RpoE is an another regulator in the expression of thin aggregative fimbriae in Salmonella [74], since the rpoE deletion mutant shows significantly reduced amounts of csgD expression and modulated biofilm formation. Compared the expression of six different Sigma factors during biofilm formation in a rpoS-independent biofilm-formation strain, the expression of rpoE gene was the highest, and the rpoE mutant could not produce biofilm [75]. Therefore, RpoE acts as a regulator for csgD expression. IHF is a histone-like heterodimeric protein composed of two homologous subunits. IHF interacts with a define DNA sequence that has a supportive A-tract upstream of the consensus sequence by binding to the minor groove of the DNA. The ihf mutants show altered and reduced biofilm morphotypes on Congo Red agar plates [72]. H-NS prefers to bind AT-rich sites in the intergenic csgBAC and csgDEFG regions and causes moderate activation of csgD promoter. The inactivation of hns gene result in reduced expression of the rdar morphotype on agar plate [72]. MlrA (MerR-like regulator) acts directly or indirectly on the csgD promoter, the mlrA mutants of Salmonella typhimurium no longer produce curli or rugose colony morphology. However, inactivation of mlrA did not affect curli production and aggregative morphology in an upregulated curli producing Salmonella typhimurium derivative containing a temperature- and RpoS-independent csgD promoter region. Therefore, MlrA acts as a positive regulator of RpoS-dependent curli and extracellular matrix production by Salmonella typhimurium [76].

c-di-GMP is recognized as a ubiquitous bacterial second messenger and a key regulator in bacterial transition from a motile and planktonic to a sessile and biofilm lifestyle. High intracellular c-di-GMP levels promote extracellular matrix production and subsequent biofilm formation and repress motility, whereas low intracellular c-di-GMP levels suppress matrix production and promote single-cell motility [77]. The synthesis/degradation of c-di-GMP depends on diguanylate cyclase/phosphodiesterase enzymatic activities. The cyclase activity, which converts two molecules of GTP to c-di-GMP, is encoded in the GGDEF protein domain, while phosphodiesterase activity, which hydrolyzes c-di-GMP to linear 5′-pGpG or two GMP molecules, is encoded in the EAL and HD-GYP domains. For example, Adar, containing a GGDEF domain, encodes diguanylate cyclase synthesizing c-di-GMP, is required for cellulose production and biofilm formation. In another seven GGDEF family (GcpA-G), only GcpA and GcpE are critical for biofilm formation [37]. The EAL domain protein STM4264, STM3611, and the GGDEF-EAL domain protein STM1703 play a determinative role in the expression level of multicellular behavior of Salmonella typhimurium [78, 79]. In contradiction, the EAL-like protein STM1697, neither degrade nor bind c-di-GMP, promotes biofilm formation and CsgD expression through interaction with proteins that regulate flagella function [80]. High intracellular amounts of c-di-GMP in Salmonella typhimurium inhibited invasion and abolished induction of a pro-inflammatory immune response in the colonic epithelial cell line HT-29. Inhibition of the invasion and IL-8 induction phenotype by c-di-GMP requires the major biofilm activator CsgD and/or BcsA. Therefore, c-di-GMP signaling is at least equally important in the regulation of Salmonella–host interaction as in the regulation of biofilm formation at ambient temperature [81].

CsgD synthesis is also regulated at the post-transcriptional level by sRNA. sRNAs have emerged as a diverse group of trans- or cis-encoded regulatory molecules of approximately 50–250 nt in size. The RNA chaperone Hfq protects sRNAs form degradation and facilitates their binding to the target mRNAs. All these sRNA may negatively regulate csgD gene expression by binding to the overlapping 5′-region of the transcript, masking the ribosome binding site, resulting in the inhibition of translation or the degradation of mRNA [82]. In Escherichia coli, sRNAs, OmrA/B, McaS, RprA, and GcvB are identified, which downregulate CsgD translation [83]. In E. coli and Salmonella, RydC’s 5′-domain interacts with csgD mRNA translation initiation signals to prevent initiation, stimulation of RydC expression reduces biofilm formation by impairing curli synthesis [84]. Surprisingly, two Hfq-dependent sRNAs (ArcZ and SdsR) are responsible for positively regulation of rdar morphotype expression in Salmonella typhimurium [85]. Salmonella biofilm development depends on the phosphorylation status of RcsB. The unphosphorylated RcsB is essential to activate the expression of the biofilm matrix compounds. The inhibition of biofilm development by phosphorylated RcsB is due to the repression of CsgD expression, through a mechanism dependent on the accumulation of the sRNA RprA [86].

Many gram-negative bacteria utilize N-acyl-L-homoserine lactones (AHLs) to bind to transcriptional regulators leading to activation or repression of target genes. Salmonella do not synthesize AHLs but do contain the AHL receptor, SdiA. The Salmonella sdiA gene regulates the rck gene, which mediates its adhesion and invasion of epithelial cells and the resistance of the organism to complement [87]. The rck gene is located on the virulence plasmid of pRST98, AHLs increase rck expression in pRST98-carrying strains, thereby enhancing bacterial adherence, serum resistance, and bacterial biofilm formation [88].

Advertisement

6. Virulence or resistance for biofilm

Biofilm formation may involve in the virulence of Salmonella. Salmonella enteritidis stains isolated from either the environment, dairy products, or infected patients are divided into two groups on the basis of their virulence (50% lethal dose) in chickens infected intraperitoneally. Only the virulent strains produce aggregates and formed visible filaments attached to the glass tube [47]. Further study confirms that the virulence of the biofilm-producing strain in infected chickens increases proportionally to the amount of stored glycogen, suggesting a possible role of the glycogen depot in the virulence of Salmonella enteritidis [89]. When tested for infection in Caco-2 cells and HEp-2 cells, the more virulent strains of Salmonella enteritidis, which are biofilm producers in adherence test medium, are able to disrupt monolayers. In contrast, the low-virulence strains of Salmonella enteritidis, which do not produce biofilms in adherence test medium, have no effect on the same cells. The high-virulence Salmonella enteritidis strains incubated under optimum biofilm-forming conditions may release a soluble factor, which enables the disruption of the integrity of Caco-2 monolayers [90]. The relationship between biofilm-forming ability and the pathogenicity is also evaluated in Salmonella pullorum. Although the virulence of Salmonella pullorum strains is independent of their ability of biofilm formation, prior growth as a biofilm for a biofilm producer of Salmonella pullorum leads to enhanced virulence in chickens, suggested that biofilm formation may be one of important virulence factor for Salmonella pullorum infection [46].

The csgBAC operon is required for curli biosynthesis in Salmonella. The csgA mutation is not reduced in ability to attach or colonize alfalfa sprouts, whereas the csgB mutation is reduced. Thus, csgB alone can play a role in attachment of Salmonella to plant tissue [91]. Competitive infection experiments in mice shows that csgA mutant cells outcompeted rdar-positive wild-type cells, indicating that aggregation via the rdar morphotype is not a virulence adaptation in Salmonella typhimurium. Furthermore, in vivo imaging experiments show that thin aggregative fimbriae genes are not expressed during infection but are expressed once Salmonella was passed out of the mice into the feces [92]. However, Salmonella typhimurium strains isolated from water buffalo calves affected by lethal gastroenteritis are tested in vivo in a mouse model of mixed infection. The most pathogenic strain is characterized by a high number of virulence factors and the presence of the locus csgA, coding for a thin aggregative fimbria [93].

The bcsABZC and bcsEFG operons are required for cellulose biosynthesis in Salmonella. Bacterial adherence and invasion assays of eukaryotic cells and in vivo virulence studies of cellulose-deficient mutants of bcsC and bcsE genes indicate that the production of cellulose is not involved in the virulence of Salmonella enteritidis. However, cellulose-deficient mutants are more sensitive to chlorine treatments, suggesting that cellulose production and biofilm formation may be an important factor for the survival of S. enteritidis on surface environments [36]. Salmonella typhimurium makes cellulose when inside macrophages. An attenuated mutant lacking the mgtC gene exhibits increased cellulose levels due to increased expression of the cellulose synthase gene bcsA and of cyclic diguanylate, the allosteric activator of the BcsA protein. Inactivation of bcsA restore wild-type virulence to the Salmonella mgtC mutant, indicating that Salmonella promotes virulence by repressing cellulose production [94].

BapA, a large cell-surface protein, is required for biofilm formation by Salmonella. Studies on the contribution of BapA to Salmonella enteritidis pathogenesis reveal that orally inoculated animals with a bapA-deficient strain survived longer than those inoculated with the wild-type strain. Also, a bapA mutant strain showed a significantly lower colonization rate at the intestinal cell barrier and consequently a decreased efficiency for organ invasion compared with the wild-type strain [26]. Osmoregulated periplasmic glucans (OPGs) are major periplasmic constituents of Gram-negative bacteria. An opgGH mutant strain in Salmonella typhimurium, which is defective in OPG biosynthesis, severely impaires biofilm formation. The opgGH mutant strain poorly colonizes mouse organs when introduced orally along with the wild-type strain [95].

Besides, the constitutional components of biofilm, there are many regulation proteins involved in both biofilm formation and virulence. An ompR mutant of Salmonella enteritidis has no ability to produce cellulose, curli, and biofilm and shows similar adherence percentage to and invasion percentage of epithelial cells as wild-type strain. Intraperitoneal challenge of bacteria in BALB/c mice reveals that the ompR mutant strain is significant attenuated [73]. A spiA gene mutant shows reduced biofilm formation and significantly decreased curli production, and reduced intracellular proliferation of macrophages during the biofilm phase. In addition, the spiA mutant was attenuated in a mouse model in both the exponential growth and biofilm phases [67]. Deletion of genes ompR and spiA in Salmonell pullorum strains contribute to attenuation of virulence in 1-day-old chickens [68]. DksA is a conserved gram-negative regulator that binds directly to the RNA polymerase secondary channel. In Salmonella typhimurium, expression of the dksA gene is induced during the logarithmic phase and DksA plays an important role in motility and biofilm formation. DksA positively regulates the Salmonella pathogenicity island 1 and motility-chemotaxis genes and is necessary for Salmonella typhimurium invasion of human epithelial cells and uptake by macrophages. The dksA gene is induced at the midcecum during the early stage of the infection and required for gastrointestinal colonization and systemic infection in a colitis mouse model [96].

Salmonella in biofilm is resistant to antibiotic. One of key mechanisms of antibiotic resistance is efflux. There are five families of multidrug resistance (MDR) efflux pumps, in which the AcrAB–TolC efflux system is the best characterized MDR system. Ten mutants of Salmonella typhimurium lacking MDR efflux systems, such as tolC, acrB, acrD, acrEF, mdtABC, mdsABC, emrAB, mdfA, mdtK, and macAB are compromised in their ability to form biofilms. The mutants expressed significantly less csgB or csgD than wild type, indicating that loss of all multidrug resistance efflux pumps of Salmonella typhimurium results in impaired ability to form a biofilm [97]. Further study confirms that mutants of Salmonella typhimurium that lack TolC or AcrB, but surprisingly not AcrA, are compromised in their ability to form biofilms. The biofilm defect results from transcriptional repression of curli biosynthesis genes and consequent inhibition of production of curli. Therefore, the inhibition of efflux is a promising antibiofilm strategy [98]. However, recent studies offer contradictory findings about the role of multidrug efflux pumps in bacterial biofilm development. When no selective pressure is applied, Salmonella typhimurium is able to produce biofilms even when the AcrAB efflux pumps are inactivated. Upon exposure to chloramphenicol, the formation of biofilms on solid surfaces as well as the production of curli are either reduced or delayed more significantly in both AcrA and AcrAB mutants, implying that the use of efflux pump inhibitors to prevent biofilm formation is not a general solution and that combined treatments might be more efficient [99]. Triclosan is a potent biocide that is included in a diverse range of products. Salmonella biofilm-derived cells are more resistant to Triclosan. Within biofilms, triclosan upregulate the transcription of acrAB, marA, bcsA, and bcsE genes. Thus, Salmonella within biofilms could experience reduced influx, increased efflux and enhanced exopolysaccharides production. The data suggest that tolerance of Salmonella towards triclosan in the biofilm is attributed to low diffusion through the extracellular matrix, while changes of gene expression might provide further resistance to triclosan and to other antimicrobials [100].

In summary, Salmonella biofilm formation is major controlled by CsgD regulatory network and regulated by multiple transcriptional factors, c-di-GMP, and sRNAs. More and more genes are found to be associated with both biofilm formation and virulence. Dissection of their function and relationship will helpful for development of new tools and strategies to prevent biofilm-related disease and decontaminate biofilm-derived Salmonella in food production.

References

  1. 1. Popoff MY, Bockemuhl J, Gheesling LL. Supplement 2002 (no. 46) to the Kauffmann-White scheme. Res Microbiol 2004,155:568–570.
  2. 2. Foley SL, Lynne AM, Nayak R. Salmonella challenges: prevalence in swine and poultry and potential pathogenicity of such isolates. J Anim Sci 2008,86:E149–162.
  3. 3. Uzzau S, Brown DJ, Wallis T, Rubino S, Leori G, Bernard S, et al. Host adapted serotypes of Salmonella enterica. Epidemiol Infect 2000,125:229–255.
  4. 4. Majowicz SE, Musto J, Scallan E, Angulo FJ, Kirk M, O’Brien SJ, et al. The global burden of nontyphoidal Salmonella gastroenteritis. Clin Infect Dis 2010,50:882–889.
  5. 5. Pires SM, Vieira AR, Hald T, Cole D. Source attribution of human salmonellosis: an overview of methods and estimates. Foodborne Pathog Dis 2014,11:667–676.
  6. 6. Marin C, Hernandiz A, Lainez M. Biofilm development capacity of Salmonella strains isolated in poultry risk factors and their resistance against disinfectants. Poult Sci 2009,88:424–431.
  7. 7. Scher K, Romling U, Yaron S. Effect of heat, acidification, and chlorination on Salmonella enterica serovar typhimurium cells in a biofilm formed at the air-liquid interface. Appl Environ Microbiol 2005,71:1163–1168.
  8. 8. Joseph B, Otta SK, Karunasagar I, Karunasagar I. Biofilm formation by salmonella spp. on food contact surfaces and their sensitivity to sanitizers. Int J Food Microbiol 2001,64:367–372.
  9. 9. Gonzalez-Escobedo G, Marshall JM, Gunn JS. Chronic and acute infection of the gall bladder by Salmonella typhi: understanding the carrier state. Nat Rev Microbiol 2011,9:9–14.
  10. 10. Gonzalez-Escobedo G, Gunn JS. Identification of Salmonella enterica serovar Typhimurium genes regulated during biofilm formation on cholesterol gallstone surfaces. Infect Immun 2013,81:3770–3780.
  11. 11. Donlan RM. Biofilm formation: a clinically relevant microbiological process. Clin Infect Dis 2001,33:1387–1392.
  12. 12. Barnhart MM, Chapman MR. Curli biogenesis and function. Annu Rev Microbiol 2006,60:131–147.
  13. 13. Gjermansen M, Ragas P, Sternberg C, Molin S, Tolker-Nielsen T. Characterization of starvation-induced dispersion in Pseudomonas putida biofilms. Environ Microbiol 2005,7:894–906.
  14. 14. Barak JD, Jahn CE, Gibson DL, Charkowski AO. The role of cellulose and O-antigen capsule in the colonization of plants by Salmonella enterica. Mol Plant Microbe Interact 2007,20:1083–1091.
  15. 15. Brandl MT. Fitness of human enteric pathogens on plants and implications for food safety. Annu Rev Phytopathol 2006,44:367–392.
  16. 16. Hood SK, Zottola EA. Adherence to stainless steel by foodborne microorganisms during growth in model food systems. Int J Food Microbiol 1997,37:145–153.
  17. 17. Momba MN, Kaleni P. Regrowth and survival of indicator microorganisms on the surfaces of household containers used for the storage of drinking water in rural communities of South Africa. Water Res 2002,36:3023–3028.
  18. 18. Wang H, Ding S, Dong Y, Ye K, Xu X, Zhou G. Biofilm formation of Salmonella serotypes in simulated meat processing environments and its relationship to cell characteristics. J Food Prot 2013,76:1784–1789.
  19. 19. Solomon EB, Niemira BA, Sapers GM, Annous BA. Biofilm formation, cellulose production, and curli biosynthesis by Salmonella originating from produce, animal, and clinical sources. J Food Prot 2005,68:906–912.
  20. 20. Prouty AM, Schwesinger WH, Gunn JS. Biofilm formation and interaction with the surfaces of gallstones by Salmonella spp. Infect Immun 2002,70:2640–2649.
  21. 21. Marshall JM, Flechtner AD, La Perle KM, Gunn JS. Visualization of extracellular matrix components within sectioned Salmonella biofilms on the surface of human gallstones. Plos One 2014,9:e89243.
  22. 22. Ledeboer NA, Jones BD. Exopolysaccharide sugars contribute to biofilm formation by Salmonella enterica serovar typhimurium on HEp-2 cells and chicken intestinal epithelium. J Bacteriol 2005,187:3214–3226.
  23. 23. Boddicker JD, Ledeboer NA, Jagnow J, Jones BD, Clegg S. Differential binding to and biofilm formation on, HEp-2 cells by Salmonella enterica serovar Typhimurium is dependent upon allelic variation in the fimH gene of the fim gene cluster. Mol Microbiol 2002,45:1255–1265.
  24. 24. Gerstel U, Romling U. The csgD promoter, a control unit for biofilm formation in Salmonella typhimurium. Res Microbiol 2003,154:659–667.
  25. 25. Romling U. Characterization of the rdar morphotype, a multicellular behaviour in Enterobacteriaceae. Cell Mol Life Sci 2005,62:1234–1246.
  26. 26. Latasa C, Roux A, Toledo-Arana A, Ghigo JM, Gamazo C, Penades JR, et al. BapA, a large secreted protein required for biofilm formation and host colonization of Salmonella enterica serovar Enteritidis. Mol Microbiol 2005,58:1322–1339.
  27. 27. Gibson DL, White AP, Snyder SD, Martin S, Heiss C, Azadi P, et al. Salmonella produces an O-antigen capsule regulated by AgfD and important for environmental persistence. J Bacteriol 2006,188:7722–7730.
  28. 28. Johnson L, Horsman SR, Charron-Mazenod L, Turnbull AL, Mulcahy H, Surette MG, et al. Extracellular DNA-induced antimicrobial peptide resistance in Salmonella enterica serovar Typhimurium. BMC Microbiol 2013,13:115.
  29. 29. Wang H, Huang Y, Wu S, Li Y, Ye Y, Zheng Y, et al. Extracellular DNA inhibits Salmonella enterica Serovar Typhimurium and S. enterica Serovar Typhi biofilm development on abiotic surfaces. Curr Microbiol 2014,68:262–268.
  30. 30. Romling U, Bokranz W, Rabsch W, Zogaj X, Nimtz M, Tschape H. Occurrence and regulation of the multicellular morphotype in Salmonella serovars important in human disease. Int J Med Microbiol 2003,293:273–285.
  31. 31. Romling U, Bian Z, Hammar M, Sierralta WD, Normark S. Curli fibers are highly conserved between Salmonella typhimurium and Escherichia coli with respect to operon structure and regulation. J Bacteriol 1998,180:722–731.
  32. 32. Collinson SK, Clouthier SC, Doran JL, Banser PA, Kay WW. Salmonella enteritidis agfBAC operon encoding thin, aggregative fimbriae. J Bacteriol 1996,178:662–667.
  33. 33. Gibson DL, White AP, Rajotte CM, Kay WW. AgfC and AgfE facilitate extracellular thin aggregative fimbriae synthesis in Salmonella enteritidis. Microbiology 2007,153:1131–1140.
  34. 34. Giaouris E, Samoilis G, Chorianopoulos N, Ercolini D, Nychas GJ. Differential protein expression patterns between planktonic and biofilm cells of Salmonella enterica serovar Enteritidis PT4 on stainless steel surface. Int J Food Microbiol 2013,162:105–113.
  35. 35. Romling U. Molecular biology of cellulose production in bacteria. Res Microbiol 2002,153:205–212.
  36. 36. Solano C, Garcia B, Valle J, Berasain C, Ghigo JM, Gamazo C, et al. Genetic analysis of Salmonella enteritidis biofilm formation: critical role of cellulose. Mol Microbiol 2002,43:793–808.
  37. 37. Garcia B, Latasa C, Solano C, Garcia-del Portillo F, Gamazo C, Lasa I. Role of the GGDEF protein family in Salmonella cellulose biosynthesis and biofilm formation. Mol Microbiol 2004,54:264–277.
  38. 38. Simm R, Fetherston JD, Kader A, Romling U, Perry RD. Phenotypic convergence mediated by GGDEF-domain-containing proteins. J Bacteriol 2005,187:6816–6823.
  39. 39. Latasa C, Solano C, Penades JR, Lasa I. Biofilm-associated proteins. C R Biol 2006,329:849–857.
  40. 40. Biswas R, Agarwal RK, Bhilegaonkar KN, Kumar A, Nambiar P, Rawat S, et al. Cloning and sequencing of biofilm-associated protein (bapA) gene and its occurrence in different serotypes of Salmonella. Lett Appl Microbiol 2011,52:138–143.
  41. 41. Anriany YA, Weiner RM, Johnson JA, De Rezende CE, Joseph SW. Salmonella enterica serovar Typhimurium DT104 displays a rugose phenotype. Appl Environ Microbiol 2001,67:4048–4056.
  42. 42. Crawford RW, Gibson DL, Kay WW, Gunn JS. Identification of a bile-induced exopolysaccharide required for Salmonella biofilm formation on gallstone surfaces. Infect Immun 2008,76:5341–5349.
  43. 43. O’Toole GA, Kolter R. Initiation of biofilm formation in Pseudomonas fluorescens WCS365 proceeds via multiple, convergent signalling pathways: a genetic analysis. Mol Microbiol 1998,28:449–461.
  44. 44. Vandecandelaere I, Van Acker H, Coenye T. A microplate-based system as in vitro model of biofilm growth and quantification. Methods Mol Biol 2016,1333:53–66.
  45. 45. Burton E, Yakandawala N, LoVetri K, Madhyastha MS. A microplate spectrofluorometric assay for bacterial biofilms. J Ind Microbiol Biotechnol 2007,34:1–4.
  46. 46. Lu Y, Dong H, Chen S, Chen Y, Peng D, Liu X. Characterization of Biofilm formation by Salmonella enterica Serovar Pullorum Strains. Afr J Microbiol Res 2011,5:9.
  47. 47. Solano C, Sesma B, Alvarez M, Humphrey TJ, Thorns CJ, Gamazo C. Discrimination of strains of Salmonella enteritidis with differing levels of virulence by an in vitro glass adherence test. J Clin Microbiol 1998,36:674–678.
  48. 48. Harrison-Balestra C, Cazzaniga AL, Davis SC, Mertz PM. A wound-isolated Pseudomonas aeruginosa grows a biofilm in vitro within 10 hours and is visualized by light microscopy. Dermatol Surg 2003,29:631–635.
  49. 49. Anriany Y, Sahu SN, Wessels KR, McCann LM, Joseph SW. Alteration of the rugose phenotype in waaG and ddhC mutants of Salmonella enterica serovar Typhimurium DT104 is associated with inverse production of curli and cellulose. Appl Environ Microbiol 2006,72:5002–5012.
  50. 50. Malcova M, Hradecka H, Karpiskova R, Rychlik I. Biofilm formation in field strains of Salmonella enterica serovar Typhimurium: identification of a new colony morphology type and the role of SGI1 in biofilm formation. Vet Microbiol 2008,129:360–366.
  51. 51. Niemira BA, Solomon EB. Sensitivity of planktonic and biofilm-associated Salmonella spp. to ionizing radiation. Appl Environ Microbiol 2005,71:2732–2736.
  52. 52. Hultgren SJ, Normark S, Abraham SN. Chaperone-assisted assembly and molecular architecture of adhesive pili. Annu Rev Microbiol 1991,45:383–415.
  53. 53. Baumler AJ, Tsolis RM, Heffron F. The lpf fimbrial operon mediates adhesion of Salmonella typhimurium to murine Peyer’s patches. Proc Natl Acad Sci USA 1996,93:279–283.
  54. 54. Baumler AJ, Winter SE, Thiennimitr P, Casadesus J. Intestinal and chronic infections: Salmonella lifestyles in hostile environments. Environ Microbiol Rep 2011,3:508–517.
  55. 55. Ledeboer NA, Frye JG, McClelland M, Jones BD. Salmonella enterica serovar Typhimurium requires the Lpf, Pef, and Tafi fimbriae for biofilm formation on HEp-2 tissue culture cells and chicken intestinal epithelium. Infect Immun 2006,74:3156–3169.
  56. 56. Austin JW, Sanders G, Kay WW, Collinson SK. Thin aggregative fimbriae enhance Salmonella enteritidis biofilm formation. FEMS Microbiol Lett 1998,162:295–301.
  57. 57. Raghunathan D, Wells TJ, Morris FC, Shaw RK, Bobat S, Peters SE, et al. SadA, a trimeric autotransporter from Salmonella enterica serovar Typhimurium, can promote biofilm formation and provides limited protection against infection. Infect Immun 2011,79:4342–4352.
  58. 58. Kroupitski Y, Brandl MT, Pinto R, Belausov E, Tamir-Ariel D, Burdman S, et al. Identification of Salmonella enterica genes with a role in persistence on lettuce leaves during cold storage by recombinase-based in vivo expression technology. Phytopathology 2013,103:362–372.
  59. 59. Romling U, Rohde M. Flagella modulate the multicellular behavior of Salmonella typhimurium on the community level. FEMS Microbiol Lett 1999,180:91–102.
  60. 60. Kim SH, Wei CI. Molecular characterization of biofilm formation and attachment of Salmonella enterica serovar Typhimurium DT104 on food contact surfaces. J Food Prot 2009,72:1841–1847.
  61. 61. Crawford RW, Reeve KE, Gunn JS. Flagellated but not hyperfimbriated Salmonella enterica serovar Typhimurium attaches to and forms biofilms on cholesterol-coated surfaces. J Bacteriol 2010,192:2981–2990.
  62. 62. Jennings ME, Quick LN, Ubol N, Shrom S, Dollahon N, Wilson JW. Characterization of Salmonella type III secretion hyper-activity which results in biofilm-like cell aggregation. Plos One 2012,7:e33080.
  63. 63. Ban GH, Kang DH, Yoon H. Transcriptional response of selected genes of Salmonella enterica serovar Typhimurium biofilm cells during inactivation by superheated steam. Int J Food Microbiol 2015,192:117–123.
  64. 64. Hamilton S, Bongaerts RJ, Mulholland F, Cochrane B, Porter J, Lucchini S, et al. The transcriptional programme of Salmonella enterica serovar Typhimurium reveals a key role for tryptophan metabolism in biofilms. BMC Genom 2009,10:599.
  65. 65. Malcova M, Karasova D, Rychlik I. aroA and aroD mutations influence biofilm formation in Salmonella enteritidis. FEMS Microbiol Lett 2009,291:44–49.
  66. 66. Dong H, Zhang X, Pan Z, Peng D, Liu X. Identification of genes for biofilm formation in a Salmonella enteritidis strain by transposon mutagenesis. Wei Sheng Wu Xue Bao 2008,48:869–873.
  67. 67. Dong H, Peng D, Jiao X, Zhang X, Geng S, Liu X. Roles of the spiA gene from Salmonella enteritidis in biofilm formation and virulence. Microbiology 2011,157:1798–1805.
  68. 68. Lu Y, Chen S, Dong H, Sun H, Peng D, Liu X. Identification of genes responsible for biofilm formation or virulence in Salmonella enterica serovar pullorum. Avian Dis 2012,56:134–143.
  69. 69. Liu Z, Niu H, Wu S, Huang R. CsgD regulatory network in a bacterial trait-altering biofilm formation. Emerg Microbes Infect 2014,3:e1.
  70. 70. Zakikhany K, Harrington CR, Nimtz M, Hinton JC, Romling U. Unphosphorylated CsgD controls biofilm formation in Salmonella enterica serovar Typhimurium. Mol Microbiol 2010,77:771–786.
  71. 71. Romling U, Sierralta WD, Eriksson K, Normark S. Multicellular and aggregative behaviour of Salmonella typhimurium strains is controlled by mutations in the agfD promoter. Mol Microbiol 1998,28:249–264.
  72. 72. Gerstel U, Park C, Romling U. Complex regulation of csgD promoter activity by global regulatory proteins. Mol Microbiol 2003,49:639–654.
  73. 73. Dong H, Peng D, Jiao X, Zhang X, Chen S, Lu Y, et al. Construction and characterization of an ompR gene deletion mutant from Salmonella enteritidis. Wei Sheng Wu Xue Bao 2011,51:1256–1262.
  74. 74. Yoo AY, Yu JE, Yoo H, Lee TH, Lee WH, Oh JI, et al. Role of sigma factor E in regulation of Salmonella Agf expression. Biochem Biophys Res Commun 2013,430:131–136.
  75. 75. Huang J, Chen S, Huang K, Yang L, Wu B, Peng D. Identification of rpoE gene associated with biofilm formation of Salmonella pullorum. Wei Sheng Wu Xue Bao 2015,55:156–163.
  76. 76. Brown PK, Dozois CM, Nickerson CA, Zuppardo A, Terlonge J, Curtiss R, 3rd. MlrA, a novel regulator of curli (AgF) and extracellular matrix synthesis by Escherichia coli and Salmonella enterica serovar Typhimurium. Mol Microbiol 2001,41:349–363.
  77. 77. Romling U, Gomelsky M, Galperin MY. C-di-GMP: the dawning of a novel bacterial signalling system. Mol Microbiol 2005,57:629–639.
  78. 78. Simm R, Lusch A, Kader A, Andersson M, Romling U. Role of EAL-containing proteins in multicellular behavior of Salmonella enterica serovar Typhimurium. J Bacteriol 2007,189:3613–3623.
  79. 79. Jonas K, Edwards AN, Ahmad I, Romeo T, Romling U, Melefors O. Complex regulatory network encompassing the Csr, c-di-GMP and motility systems of Salmonella typhimurium. Environ Microbiol 2010,12:524–540.
  80. 80. Ahmad I, Wigren E, Le Guyon S, Vekkeli S, Blanka A, El Mouali Y, et al. The EAL-like protein STM1697 regulates virulence phenotypes, motility and biofilm formation in Salmonella typhimurium. Mol Microbiol 2013,90:1216–1232.
  81. 81. Ahmad I, Lamprokostopoulou A, Le Guyon S, Streck E, Barthel M, Peters V, et al. Complex c-di-GMP signaling networks mediate transition between virulence properties and biofilm formation in Salmonella enterica serovar Typhimurium. Plos One 2011,6:e28351.
  82. 82. Mika F, Hengge R. Small regulatory RNAs in the control of motility and biofilm formation in E. coli and Salmonella. Int J Mol Sci 2013,14:4560–4579.
  83. 83. Boehm A, Vogel J. The csgD mRNA as a hub for signal integration via multiple small RNAs. Mol Microbiol 2012,84:1–5.
  84. 84. Bordeau V, Felden B. Curli synthesis and biofilm formation in enteric bacteria are controlled by a dynamic small RNA module made up of a pseudoknot assisted by an RNA chaperone. Nucleic Acids Res 2014,42:4682–4696.
  85. 85. Monteiro C, Papenfort K, Hentrich K, Ahmad I, Le Guyon S, Reimann R, et al. Hfq and Hfq-dependent small RNAs are major contributors to multicellular development in Salmonella enterica serovar Typhimurium. RNA Biol 2012,9:489–502.
  86. 86. Latasa C, Garcia B, Echeverz M, Toledo-Arana A, Valle J, Campoy S, et al. Salmonella biofilm development depends on the phosphorylation status of RcsB. J Bacteriol 2012,194:3708–3722.
  87. 87. Smith JL, Fratamico PM, Yan X. Eavesdropping by bacteria: the role of SdiA in Escherichia coli and Salmonella enterica serovar Typhimurium quorum sensing. Foodborne Pathog Dis 2011,8:169–178.
  88. 88. Liu Z, Que F, Liao L, Zhou M, You L, Zhao Q, et al. Study on the promotion of bacterial biofilm formation by a Salmonella conjugative plasmid and the underlying mechanism. Plos One 2014,9:e109808.
  89. 89. Bonafonte MA, Solano C, Sesma B, Alvarez M, Montuenga L, Garcia-Ros D, et al. The relationship between glycogen synthesis, biofilm formation and virulence in Salmonella enteritidis. FEMS Microbiol Lett 2000,191:31–36.
  90. 90. Solano C, Sesma B, Alvarez M, Urdaneta E, Garcia-Ros D, Calvo A, et al. Virulent strains of Salmonella enteritidis disrupt the epithelial barrier of Caco-2 and HEp-2 cells. Arch Microbiol 2001,175:46–51.
  91. 91. Barak JD, Gorski L, Naraghi-Arani P, Charkowski AO. Salmonella enterica virulence genes are required for bacterial attachment to plant tissue. Appl Environ Microbiol 2005,71:5685–5691.
  92. 92. White AP, Gibson DL, Grassl GA, Kay WW, Finlay BB, Vallance BA, et al. Aggregation via the red, dry, and rough morphotype is not a virulence adaptation in Salmonella enterica serovar Typhimurium. Infect Immun 2008,76:1048–1058.
  93. 93. Borriello G, Lucibelli MG, Pesciaroli M, Carullo MR, Graziani C, Ammendola S, et al. Diversity of Salmonella spp. serovars isolated from the intestines of water buffalo calves with gastroenteritis. BMC Vet Res 2012,8:201.
  94. 94. Pontes MH, Lee EJ, Choi J, Groisman EA. Salmonella promotes virulence by repressing cellulose production. Proc Natl Acad Sci USA 2015,112:5183–5188.
  95. 95. Liu L, Tan S, Jun W, Smith A, Meng J, Bhagwat AA. Osmoregulated periplasmic glucans are needed for competitive growth and biofilm formation by Salmonella enterica serovar Typhimurium in leafy-green vegetable wash waters and colonization in mice. FEMS Microbiol Lett 2009,292:13–20.
  96. 96. Azriel S, Goren A, Rahav G, Gal-Mor O. The stringent response regulator DksA is required for Salmonella enterica serovar Typhimurium growth in minimal medium, motility, biofilm formation, and intestinal colonization. Infect Immun 2015,84:375–384.
  97. 97. Baugh S, Ekanayaka AS, Piddock LJ, Webber MA. Loss of or inhibition of all multidrug resistance efflux pumps of Salmonella enterica serovar Typhimurium results in impaired ability to form a biofilm. J Antimicrob Chemother 2012,67:2409–2417.
  98. 98. Baugh S, Phillips CR, Ekanayaka AS, Piddock LJ, Webber MA. Inhibition of multidrug efflux as a strategy to prevent biofilm formation. J Antimicrob Chemother 2014,69:673–681.
  99. 99. Schlisselberg DB, Kler E, Kisluk G, Shachar D, Yaron S. Biofilm formation ability of Salmonella enterica serovar Typhimurium acrAB mutants. Int J Antimicrob Agents 2015,46:456–459.
  100. 100. Tabak M, Scher K, Hartog E, Romling U, Matthews KR, Chikindas ML, et al. Effect of triclosan on Salmonella typhimurium at different growth stages and in biofilms. FEMS Microbiol Lett 2007,267:200–206.

Written By

Daxin Peng

Submitted: 23 October 2015 Reviewed: 07 March 2016 Published: 13 July 2016