Biology of Streptococcus mutans-Derived Glucosyltransferases: Role in Extracellular Matrix Formation of Cariogenic BiofilmsBowen W.H.a, b · Koo H.a, b, c
aCenter for Oral Biology, bDepartment of Microbiology and Immunology and cEastman Department of Dentistry, University of Rochester, Rochester, N.Y., USA Corresponding Author
The importance of Streptococcus mutans in the etiology and pathogenesis of dental caries is certainly controversial, in part because excessive attention is paid to the numbers of S. mutans and acid production while the matrix within dental plaque has been neglected. S. mutans does not always dominate within plaque; many organisms are equally acidogenic and aciduric. It is also recognized that glucosyltransferases from S. mutans (Gtfs) play critical roles in the development of virulent dental plaque. Gtfs adsorb to enamel synthesizing glucans in situ, providing sites for avid colonization by microorganisms and an insoluble matrix for plaque. Gtfs also adsorb to surfaces of other oral microorganisms converting them to glucan producers. S. mutans expresses 3 genetically distinct Gtfs; each appears to play a different but overlapping role in the formation of virulent plaque. GtfC is adsorbed to enamel within pellicle whereas GtfB binds avidly to bacteria promoting tight cell clustering, and enhancing cohesion of plaque. GtfD forms a soluble, readily metabolizable polysaccharide and acts as a primer for GtfB. The behavior of soluble Gtfs does not mirror that observed with surface-adsorbed enzymes. Furthermore, the structure of polysaccharide matrix changes over time as a result of the action of mutanases and dextranases within plaque. Gtfs at distinct loci offer chemotherapeutic targets to prevent caries. Nevertheless, agents that inhibit Gtfs in solution frequently have a reduced or no effect on adsorbed enzymes. Clearly, conformational changes and reactions of Gtfs on surfaces are complex and modulate the pathogenesis of dental caries in situ, deserving further investigation.
Copyright © 2011 S. Karger AG, Basel
Put simply, there is no biofilm without an extracellular polysaccharide (EPS) matrix [Flemming and Wingender, 2010]. The word ‘plaque’ in a dental context was probably first used by Black  when he described the collective accumulation of microorganisms on early carious lesions. Dental plaque, which has endured various definitions, is clearly a biofilm, i.e. a group of microorganisms embedded in a matrix attached to the tooth surface. All biofilms have at least one property in common, i.e. the presence of a bacterially derived matrix [Flemming and Wingender, 2010]. The structure, e.g. branching of EPS and, to a lesser extent, the composition (e.g. proportions of soluble and insoluble polymers) of the matrix may be as variable as the microbial constituents and is influenced by local environmental conditions and even changes with time [Branda et al., 2005]. Clearly the structure of the polysaccharide matrix can play a critical role affecting the virulence of plaque by influencing the physical and biochemical properties of biofilm. It may enhance adherence of microorganisms, promote coherence, act as reserve source of energy, protect microorganisms from inimical influences, affect diffusion of substances into and out of biofilm, and help to concentrate metal ions and other physiological nutrients within a microenvironment [Tatevossian, 1990; Wilson and Ashley, 1990; Hayacibara et al., 2004; Paes Leme et al., 2006; Flemming and Wingender, 2010; Koo et al., 2010b].
Composition of Dental Plaque
The broad composition of the biofilm known as dental plaque has been explored. Glucan (see below) comprises 10–20% dry weight of dental plaque and fructan approximately 1–2%; clearly these proportions will vary depending in part at least on the duration since the last intake of food [Critchley et al., 1967; Gibbons, 1968; Wood, 1969; Mayhall and Butler, 1976; Emilson et al., 1984]. Dental plaque also contains approximately 40% dry weight protein (mostly derived from bacteria and saliva), variable amounts of lipid, Ca, P, Mg and F compared with surrounding saliva [Hotz et al., 1972; Cole and Bowen, 1975; Paes Leme et al., 2006; Pessan et al., 2008]. Dental plaque in situharbors approximately 80% water [Wilson and Ashley, 1990].
Electron histochemistry and transmission electron microscopy of dental plaque reveals microorganisms embedded in a matrix of polysaccharide [McDougall, 1963; Reese and Guggenheim, 2007], which appears to increase following exposure to sucrose [Saxton and Kolendo, 1967; Critchley et al., 1968]. All the available evidence shows clearly that the primary sources of EPS in dental plaque are products from the interaction of glucosyltransferases (Gtfs) and fructosyltransferases with sucrose and starch hydrolysates [Vacca-Smith et al., 1996a].
Role of Gtfs in Dental Plaque Formation
The earliest evidence of plaque formation is the appearance of a pellicle on the tooth surface [Leach and Saxton, 1966; Hay, 1967; Siqueira et al., 2007]. This material is repeatedly referred to as salivary pellicle even though it is clear that the pellicle harbors significant amounts of nonmammalian constituents [Eggen and Rölla, 1983; Rölla et al., 1983a; Vacca-Smith and Bowen, 1998; Hannig et al., 2008a] which influence the subsequent development of plaque. The saliva-derived constituents are selectively adsorbed to the surface, and include but are not limited to proline-rich proteins, amylase, lysozyme, histatins, peroxidase, statherin and mucin 2 [Mayhall and Butler, 1976; Siqueira et al., 2007]. Some of these materials undergo conformational change when adsorbed to tooth surfaces and may then provide specific binding sites for some microorganisms [Hay et al., 1971; Gibbons et al., 1990].
The presence of bacterial cellular material in pellicle was reported by Armstrong , but it remained for Rölla et al. [1983a] and Scheie et al.  to identify the presence of soluble bacterial products in pellicle using immunological techniques. They identified fructosyltransferase, Gtf and lipoteichoic acid in pellicle formed in vitro and in vivo from whole saliva. These observations were subsequently confirmed and extended by Vacca-Smith et al. [1996b] in pellicles formed on apatitic surface in situ. The Gtfs present in pellicle were shown by Schilling and Bowen  to be active and capable of synthesizing glucan in situ from sucrose and provided binding sites for many oral microorganisms, including mutans streptococci. Gtfs present in whole saliva are incorporated into pellicle and form part of its structure; furthermore, Gtf added to ductal saliva (Gtf-free) is also adsorbed in active form onto hydroxyapatite (HA) surfaces [Schilling and Bowen, 1988]. Remarkably, Gtf incorporated into pellicle adsorbed to an HA surface displayed 3–4 times enhanced activity compared with similar amounts of enzyme in solution [Schilling et al., 1989; Venkitaraman et al., 1995; Vacca-Smith et al., 1996b].
Furthermore, it was observed that the enzymes when insolubilized remained highly active over a wide range of pH values [Schilling and Bowen, 1988; Venkitaraman et al., 1995; Vacca-Smith et al., 1996b]. It is clear that the presence of active Gtf within dental pellicle facilitates the formation of glucan in situ, thereby providing distinct binding sites for oral microorganisms. It can therefore be hypothesized that Gtfs from S. mutans influence the microbial colonization of tooth surfaces.
Gtf can be readily assayed in whole saliva from many persons, particularly those who are caries active [Scheie and Rölla, 1986; Scheie et al., 1987; Vacca-Smith et al., 2007]. Gtfs are remarkably stable even in whole saliva; measured amounts of purified Gtf enzymes added to whole saliva remained completely active for up to 4 h at least [Vacca-Smith et al., 1996b]. Several groups of oral microorganisms produce Gtfs; these include Streptococcus sanguinis, Streptococcus mutans, Streptococcus sobrinus, Actinomyces spp., Streptococcus salivarius and Lactobacillus spp. [Newbrun, 1974]. The review presented here will focus on the Gtfs from S. mutans.
S. mutans produces at least 3 genetically separate Gtfs, each of which synthesizes a structurally distinct glucan from sucrose. Details of the structural and functional organization of Gtfs are found elsewhere [for reviews, see Monchois et al., 1999; van Hijum et al., 2006]. GtfB (formally known as GtfI) synthesizes primarily insoluble glucan rich in α-1,3-linkages, GtfC (GtfSI) produces a mixture of soluble (with mostly α-1,6-linkages) and insoluble glucans, and GtfD (GtfS) forms predominantly soluble glucans [Aoki et al., 1986; Hanada and Kuramitsu, 1988, 1989]. Superficially, it may appear bizarre that microorganisms produce 3 distinct enzymes to act on the same substrate to form polysaccharides. We hypothesize with supporting data that each one plays a distinct role in the formation of dental plaque and, as a result, S. mutans has a far greater influence on the formation and composition of plaque than its population would appear to warrant.
Gtf adsorbs to experimental pellicles formed on apatitic surfaces in situ with extraordinary rapidity; active Gtf is detected on HA disks within 1 min of placing them in the mouth. Prerinsing with sucrose enhances the amount of enzyme detected, possibly because Gtf will adhere to glucan formed in situ [Scheie et al., 1987; Vacca-Smith and Bowen, 2000]. In vitro, Gtf binds poorly to uncoated HA and loses much of its activity [Schilling and Bowen, 1988; Vacca-Smith and Bowen, 1998]; in contrast, Gtf adsorbs to saliva-coated HA (sHA) disks avidly with enhanced activity [Venkitaraman et al., 1995; Steinberg et al., 1996].
Results from early studies, before separate gene products were available, provided little information on which Gtf is present in pellicle [Schilling and Bowen, 1988]. As a result of cloning and gene deletion, the Gtf enzymes have been prepared separately and at a high level of purity which has led to rapid advances in the field [Hanada and Kuramitsu, 1988; Fukushima et al., 1992]. Although all 3 enzymes can bind to sHA, their affinity differs greatly [Vacca-Smith and Bowen, 1998]. GtfC has the greatest affinity for sHA, and in addition, based on Scatchard plots, GtfC displayed significantly more binding sites than did either GtfB or GtfD. Although GtfD binds to sHA, it displays relatively few binding sites. It is also noteworthy that the Km values for the 3 enzymes are lower by two- to eightfold following adsorption to sHA, an observation consistent with the reported enhanced activity of the insolubilized enzymes compared with the same enzymes in solution [Kuramitsu and Ingersoll, 1978; Venkitaraman et al., 1995; Steinberg et al., 1996]. The activity of GtfB is enhanced greatly by the inclusion of primer dextran in the test system [Koga et al., 1988; Venkitaraman et al., 1995; Vacca-Smith et al., 1996a; Kopec et al., 1997]. In contrast, Gtf detected in pellicle is not enhanced by primer dextran. Furthermore, the activity of GtfC is enhanced substantially when it is adsorbed to sHA; enhancement is not observed with GtfB adsorbed to sHA. The binding of GtfB to sHA in the presence of ductal parotid saliva supplemented with GtfC and GtfD was reduced when compared with its binding to sHA in the presence of parotid saliva alone. In contrast, the binding of GtfC or GtfD enzymes to sHA was unaffected by addition of other Gtfs [Vacca-Smith and Bowen, 2000]. We conclude therefore that the Gtf in pellicle has properties that are certainly consistent with it being GtfC [Vacca-Smith et al., 1996b]. Data from in situ and in vitro studies suggest strongly that Gtf detected in pellicle is primarily GtfC from S. mutans [Venkitaraman et al., 1995; Vacca-Smith and Bowen, 2000].
Gtfs also have the capacity to bind to many oral bacteria [McCabe and Donkersloot, 1977; Hamada et al., 1978; Vacca-Smith and Bowen, 1998], even those that do not synthesize Gtfs. We have observed that GtfB binds with greater avidity to oral microorganisms, e.g. Actinomyces viscosus, Lactobacillus casei and S. mutans, than do the other Gtfs from S. mutans and that the binding to bacteria occurs even in the presence of ductal saliva. Furthermore, the enzyme retains its activity when adsorbed to bacteria, thereby converting non-Gtf producers into de facto glucan formers [Vacca-Smith and Bowen, 1998].
The simultaneous synthesis of glucans by surface-adsorbed GtfB and GtfC is essential for the establishment of a matrix that enhances the coherence of bacterial cells and adherence to apatitic surfaces, allowing the formation of highly organized and dense cell clusters known as microcolonies [Tamesada et al., 2004; Koo et al., 2010b; Xiao and Koo, 2010]. These phenomena may well explain the observations on histochemical preparations of even early plaque that reveal microorganisms embedded in a polysaccharide matrix [Critchley et al., 1968; Venkitaraman et al., 1995; Reese and Guggenheim, 2007].
The precise mechanisms involved in the binding of Gtfs to sHA and bacterial surfaces remain to be elucidated. The same type of basic structure is found in all Gtfs [Russell et al., 1988; Russell, 1994; Vacca-Smith and Bowen, 1998]. Each enzyme has at the amino terminus a signal peptide comprised of approximately 38 amino acids; adjacent to this peptide is a very variable domain constituted by about 200 amino acids characteristic for each of the enzymes [van Hijum et al., 2006]. The amino acid composition and structure of the Gtfs may clarify the distinct binding capacities of each enzyme.
A series of repeat motifs of amino acids that varies for each enzyme is found at the C terminus. The C termini found in GtfB and GtfC differ in composition, which may explain in part at least the preferential adsorption of GtfC enzyme to sHA and of GtfB enzyme to bacterial surfaces. The GtfB and GtfD are comparable in structure and both are hydrophilic [Shiroza et al., 1987; Honda et al., 1990]. GtfC is also hydrophilic; however, in contrast to the GtfB and GtfD enzymes, it harbors a hydrophobic domain within the direct repeat units in the C terminus [Ueda et al., 1988]. The presence of small hydrophobic domains in GtfC may be associated with pellicle-binding activity of this enzyme, possibly through interactions with specific salivary macromolecules found in the pellicle, such as lysozyme and α-amylase [Vacca-Smith et al., 1996a; Vacca-Smith and Bowen, 1998]. Conversely, the presence of specific carboxyl-terminal repeat units of GtfB has a major role in the binding of the enzyme to the cell surface of oral streptococci [Kato and Kuramitsu, 1991].
It is noteworthy [Vickerman et al., 1996, 2003] that the ability of Gtf enzymes from S. gordonii to bind to biotin-dextran was dramatically reduced following deletion of the C-terminal hydrophilic residue. Using a series of deletion derivatives for the C terminus, it has been shown that direct repeat units constitute part of the minimum domain required for the lectin type glucan binding by S. mutans GtfD [Mooser and Wong, 1988; Lis et al., 1995]. The C-terminal glucan-binding domain of GtfD contains five 65-amino-acid direct repeat units. The removal of the single direct repeat unit significantly reduced the ability of the protein to bind glucans [Lis et al., 1995] and may be necessary for enzyme catalytic activity [van Hijum et al., 2006]. However, the precise role of the glucan-binding domain on the conformation-function relationship of Gtf enzymes, including the presumed (β/α)8 barrel structure in the catalytic domain, remains largely unknown [van Hijum et al., 2006]. Nevertheless, the tertiary structure of the glucan-binding domain (presumably containing a high percentage of β-sheet) may be essential for the lectin type glucan binding by GtfD [Mooser and Wong, 1988; Banas and Vickerman, 2003; van Hijum et al., 2006].
In addition, Gtfs also bind to other components of the salivary pellicle such as salivary peroxidase, amylase and lysozyme [Korpela et al., 2002; Hannig et al., 2005; Kho et al., 2005]. Available data shows clearly that Gtfs interact with salivary amylase in pellicle [Vacca-Smith et al., 1996a] inhibiting activity and blocking adsorption of salivary amylase to HA [Hannig et al., 2005]. Lactoperoxidase in the absence of substrates, which is structurally and enzymatically similar to salivary peroxidase, inhibits all 3 Gtf enzymes in solution or adsorbed to sHA beads [Korpela et al., 2002]. The presence of lysozyme reduced the activity of GtfB in solution and on a surface but was without apparent effect on the structure of glucan formed [Kho et al., 2005]. The interactions of Gtf with peroxidase and lysozyme in salivary pellicle could result in decreased colonization of tooth surfaces as a consequence of depressed glucan production.
It is also noteworthy that many oral microorganisms, including S. mutans, adsorb lysozyme, amylase and other salivary proteins [Douglas, 1983; Douglas and Russell, 1984; Ambatipudi et al., 2010], which may influence the binding of GtfB on the bacterial cell surface. The simultaneous binding of GtfB and salivary amylase and their interactions create the opportunity to synthesize complex insoluble glucans directly on the bacterial surface [Vacca-Smith et al., 1996a; Chaudhuri et al., 2007].
The attention to oral biofilms has been enhanced greatly in recent years largely because it is recognized that microorganisms behave differently in biofilms compared with that in the planktonic state [Marsh and Bradshaw, 1995; Hall-Stoodley et al., 2004]. Enzymes too may behave differently when adsorbed to a surface compared with solubilized enzymes [Fears and Latour, 2009]. The adsorption of Gtf to sHA results in substantial enhancement of activity compared with activity of the same enzyme in solutions [Schilling and Bowen, 1988]. In contrast to what occurs on sHA, Gtf adsorbs comparatively poorly to uncoated HA and loses some activity. Even more remarkable is the difference in structure of glucans formed by GtfB and GtfC when adsorbed to sHA compared with the product formed when the same enzyme is in solution. Based on susceptibility to dextranase and mutanase, products of digestion and structural analyses, there is a dramatic increase in the number of α-1,3-linkages and a higher percentage of 3-linked branch points (e.g. 2,3-, 3,4-, 3,6- and 3,4,6-linked glucose) in the surface-formed glucan compared with that formed by the same enzymes in solution.
The presence of starch hydrolysates, associated with gradual digestion of starch by salivary α-amylase (free in solution, adsorbed onto apatite and/or microbial surfaces), also influences the formation and structure of glucan by GtfB [Vacca-Smith et al., 1996a]. The hydrolysates, which include a range of high-molecular-weight oligomers (>1 kDa), maltotriose and maltose/isomaltose [Klein et al., 2010], can serve as acceptor sites for polymer formation, constituting an integral part of the polymer molecule [Fukui and Moriyama, 1983; Koga et al., 1988; Fu and Robyt, 1991]. Furthermore, it appears that these carbohydrates can serve as substrate for the addition of branches to glucan even in the absence of sucrose [McCabe and Hamelik, 1983]. The combination of starch hydrolysates and sucrose with surface-adsorbed GtfB results as expected in enhanced formation of predominantly insoluble glucan and an increase in the number of α-1,4- and α-1,3- linkages with 3,4-linked glucose as the major branch point [Kopec et al., 1997]. Inclusion of starch hydrolysates with sucrose is without effect on the structure of product formed by GtfC and GtfD. It is noteworthy that parts of Gtf molecules have substantial sequence similarity with members of the α-amylase family [van Hijum et al., 2006]. The significance of Gtf similarity is underlined by Gtf/α-amylase residues conserved in all but one α-amylase invariant residue [Devulappalle et al., 1997]. Moreover, the presence of amylase increased both the sucrase and transferase component activities of GtfB [Chaudhuri et al., 2007].
The product from the starch-sucrose substrate resembles in some measure the structure reported for plaque polysaccharide [Hotz et al., 1972; Birked and Rosell, 1975]. Furthermore it provides distinct binding sites for some oral microorganisms. For example, Actinomyces spp. and S. mutans bind in larger numbers to glucan formed on sHA surface in the presence of starch hydrolysates as compared to glucan formed in the absence of starch [Vacca-Smith et al., 1996a]. Sucrose is frequently consumed with starch, and this combination could clearly influence the composition, structure and physical properties of plaque matrix (more details later).
Clearly, the glucans formed on surfaces are highly insoluble, and furthermore provide distinct binding sites for microorganisms [Kopec et al., 1997] and affect the 3-dimensional structure of the matrix [Koo et al., 2010b]. Whether similar phenomena occur with glucans formed on bacterial surfaces remains to be determined.
The adherence of microorganisms to the tooth surface is critical in the formation of dental plaque, and understandably much attention has been focused on microbial binding to uncoated tooth surfaces, HA, polystyrene (plastic) or glass [Morris and McBride, 1984; Gibbons and Hay, 1989; Schilling and Bowen, 1992]. Non-pellicle-covered teeth rarely if ever occur in vivo. Salivary glycoproteins and bacterial products can be detected on HA disks within 30 s of being placed in the mouth [Hay et al., 1971; Vacca-Smith and Bowen, 2000; Hannig et al., 2008a]. Saliva-coated disks prepared in situ assayed directly for enzyme activity revealed that fructosyltransferase activity increased up to 1 min of exposure and decreased when kept in the mouth for longer periods. Gtf activity on the disks in contrast increased the longer the disks were kept in the mouth [Scheie et al., 1987; Vacca-Smith and Bowen, 2000]. Many oral microorganisms do not adhere in large numbers to uncovered HA [Schilling and Bowen, 1992] and even fewer adhere to sHA [Schilling and Bowen, 1988; Schilling et al., 1989; Venkitaraman et al., 1995; Vacca-Smith and Bowen, 1998] even though considerable selectivity is apparent, and novel binding sites in salivary glycoproteins are revealed (cryptotopes) as a result of adsorption to HA surface [Gibbons et al., 1990]. These observations on adherence are in marked contrast to what occurs when glucan is formed in situ on the surface of HA. With glucan synthesized from surface Gtfs (particularly GtfB and GtfC but not GtfD), there is a threefold increase in the number of S. mutans adhering to the glucan-coated surface compared with the number adhering to an uncoated HA or sHA surface [Kuramitsu, 1974; Schilling and Bowen, 1992; Venkitaraman et al., 1995].
The binding of S. mutans to glucans formed in situ is mediated by the presence of cell-associated Gtf enzymes and non-Gtf glucan-binding proteins (Gbps). At least 4 Gbps have been identified in S. mutans, GbpA, GbpB, GbpC and GbpD [Guggenheim, 1970; Russell, 1979; Banas and Vickerman, 2003]. GbpA and GbpD contain carboxyl-terminal repeats similar to those found in the glucan-binding domain of Gtf enzymes. The glucan-binding domain of GbpC has not been identified although it shares homology with the AgI/II family of proteins; GbpB is similar to peptidoglycan hydrolase [Banas and Vickerman, 2003]. Among them, GbpC (and possibly GbpB) is cell wall bound and may function as cell surface glucan receptors in S. mutans [Banas and Vickerman, 2003]. Each of the Gbps appears to have a role in sucrose-dependent adhesion and biofilm formation by S. mutans, although loss of cell-surface-anchored GbpC was the most disruptive [Lynch et al., 2007].
The inclusion of dextran (α-1,6-linked glucan; molecular weight 9,000) in the model system effectively blocks or reduces adherence of microorganisms to glucan-coated apatitic surface. Furthermore, treating the in situformed glucan with dextranase [Schilling et al., 1989; Venkitaraman et al., 1995] prevented or reduced bacterial adherence whereas mutanase treatment (α-1–3) was without effect. These observations suggest strongly that presence of α-1,6-linkages in GtfB- and GtfC-derived glucans is conferring a specific structure or conformation that provides at least 1 binding site.
Results from using atomic force microscopy demonstrate that attachment of S. mutans to tooth surfaces was largely mediated by glucan production and that attachment strengthens with time [Cross et al., 2007]. Evidence is lacking that ionic interactions play a role in the binding of S. mutans to glucan [Cross et al., 2007], especially considering that glucan formed in vitro is uncharged. Furthermore, it is apparent that glucan synthesized in situ by Gtf in pellicle provides enhanced binding for several oral microorganisms. Thus, it appears that a glucan surface on HA (mostly produced by GtfC) provided distinct binding sites for oral microorganisms that do not bind readily to HA or sHA. Concomitantly, glucan formed by Gtf adsorbed to the surface of cells (primarily GtfB) provides an opportunity for aggregation and accumulation of cells and structural support for development of microcolonies (fig. 1) at the same time increasing the bulk of plaque. It is apparent that the formation of cell clusters and microcolonies tightly adherent on the surface of HA is a result of interplay between GtfB and GtfC enzymes and their glucan products at different loci [Koo et al., 2010b]. The presence of highly adherent and insoluble glucans in situincreases mechanical stability by binding the bacterial cells together and to the apatite surface (fig. 1) allowing them to persist on tooth enamel in high levels for a prolonged period. These polymers, in addition to interactions with specific Gbps expressed on S. mutans (and other oral microorganisms) are critical in maintaining the 3-dimensional structure of microcolonies over time (fig. 1), thereby modulating the development of cariogenic biofilms [Lynch et al., 2007; Koo et al., 2010b; Xiao and Koo, 2010]. Based on these observations, we have revised and updated the glucan-mediated bacterial adherence model initially proposed by Rölla et al. [1983b] as shown in figure 2.
|Fig. 1.a Representative confocal images of bacterial cells (in green) and glucans (in red) within biofilms formed by S. mutans US 159 on tooth enamel surface in the presence of 1% (wt/vol) sucrose. Arrowheads indicate structural organization of glucans within microcolonies. b Close-up view of 3-dimensional structural relationship between glucans and S. mutans cells.|
|Fig. 2. Revised model of Gtf-glucan-mediated bacterial adherence and cariogenic biofilm development. Originally proposed by Rölla et al. [1983b]. (1) The Gtfs secreted by S. mutans are incorporated into pellicle (particularly GtfC) and adsorb on bacterial surfaces (mainly GtfB), including microorganisms that do not produce Gtfs (e.g. Actinomyces spp.). Furthermore, salivary α-amylase is also included into pellicle, which can also bind Gtfs. (2) Surface-adsorbed GtfB and GtfC rapidly utilize dietary sucrose to synthesize insoluble and soluble glucans in situ; the soluble glucans formed by GtfD could serve as primers for GtfB enhancing the overall synthesis of exopolysaccharides. Concomitantly, starch is digested by amylase releasing maltose and a myriad of oligosaccharides; they can be incorporated into the polymer molecule through acceptor reactions, particularly by surface-adsorbed GtfB. The Gtfs adsorbed onto enamel and microbial surfaces provide in situ an insoluble matrix for dental plaque. (3) The glucan molecules provide avid binding sites on surfaces for S. mutans (and other microorganisms) mediating tight bacterial clustering and adherence to the tooth enamel. Furthermore, Gtf-adsorbed bacteria become de facto glucan producers binding to tooth and microbial surfaces by the same mechanisms. This model could explain the rapid formation and accumulation of highly cohesive-adherent plaque in the presence of sucrose (and possibly starch) even if the number of S. mutans is relatively low. After the establishment of a glucan-rich biofilm matrix, ecological pressure (e.g. pH) will determine which bacteria may survive and dominate within plaque under frequent sucrose (or other fermentable carbohydrate) exposure.|
The precise role(s) of EPS in the pathogenesis of dental caries is in some measure controversial. Nevertheless, there is considerable agreement on many aspects [Paes Leme et al., 2006]. Glucan formed on the tooth surface synthesized by Gtf incorporated into the pellicle from sucrose can provide enhanced binding sites for a number of oral microorganisms, especially S. mutans. In turn, microorganisms that synthesize glucans, or adsorb Gtf and become de facto glucan producers, form highly stable and persistent microcolonies. The exopolymers produced in situ provide a coherent, adherent and mechanically stable matrix, and offer a continuum of a diverse range of binding sites; the structure of glucan is altered over time by the presence of mutanases and dextranases [Guggenheim and Burckhardt, 1974; Walker et al., 1981; Hayacibara et al., 2004]. In addition, Gtfs may bind to the glucan already formed within dental plaque [Tamasada et al., 2004]. Glucan adds to the bulk of plaque thereby leading to a dense concentration of microorganisms on cloistered sites of tooth surfaces protected from inimical influences [Thurnheer et al., 2003; Kreth et al., 2008; Xiao and Koo, 2010]. In addition, soluble glucans may be readily digested and used as a reserve source of energy and contribute in part at least to the low pH values observed in cariogenic plaque [as reviewed in Paes Leme et al., 2006]. It is also noteworthy that elevated amounts of insoluble glucans in dental plaque significantly reduced the inorganic concentration in the matrix, particularly Ca, P and F [Cury et al., 2000; Paes Leme et al., 2006, 2008]. Plaque should not be viewed as a homogeneous accumulation of microorganisms within a matrix but as a collection of highly organized microenvironments which can display distinct structures, compositions and diverse pH values (ranging from as low as pH 4 at the tooth-biofilm interface to as high as pH 6.5 at the biofilm-fluid phase) [Xiao et al., unpubl. data].
The physical role that glucan in plaque plays in cariogenesis is subject to diverse opinions. It is postulated that glucan limits diffusion of charged ions into and out of plaque whereas uncharged substances such as sucrose may diffuse readily [Melvaer et al., 1972, 1974; Melsen et al., 1979]. Available evidence suggests that the EPS from S. mutans and possibly additional oral microorganisms may be charged possibly by the incorporation of lipoteichoic acid [Melvaer et al., 1972, 1974; Melsen et al., 1979; Kuramitsu et al., 1980; Rölla et al., 1980; Vickerman and Jones, 1992]. In addition, Rölla et al.  have observed elevated levels of lipoteichoic acid in sucrose-induced dental plaque in vivo. Based on extensive in vitro modeling, Dibdin and Shellis  suggest that polysaccharides within plaque have little or no influence on diffusion and that spaces within the matrix of plaque provide ‘storage’ of acids and microbial products thereby providing effective maintenance of an elevated concentration of acid in contact with the tooth surface; they further suggest that this property alone may account for the virulence of the acid attack from dental plaque without invoking diffusion limitations. These observations are supported in part by Hata and Mayanagi , who noted that EPS had little effect on acid diffusion in artificial plaque. In contrast, Tatevossian  and others [Wilson and Ashley, 1990] note that concentrations of solutes in plaque fluid differ markedly from those observed in saliva, an observation which suggests that there is some restriction between the interior of dental plaque and its external environment. Furthermore, it appears that diffusion rates measured by different methods are widely diverse. Tatevossian  further notes: ‘We have much to learn about the fluid environment of the teeth and about dynamic changes in plaque fluid composition and properties during perturbations.’ Polysaccharide within dental plaque is not evenly distributed, and its density is enhanced at the tooth interface [Saxton and Kolendo, 1967; Reese and Guggenheim, 2007]. The presence of EPS-rich matrix and microcolonies appears to create a myriad of microenvironments displaying a distinct range of in situ pH values [Xiao et al., unpubl. data].
Furthermore, dietary starches and sucrose in the presence of surface-adsorbed salivary α-amylase and Gtfs enhance the formation of highly insoluble and structurally distinctive 3-dimensional matrix, increasing the accumulation of highly cohesive and adherent biofilms by S. mutans [Duarte et al., 2008; Klein et al., 2009, 2010; Xiao and Koo, 2010]. The sucrose-starch combination also induced complex remodeling of S. mutans transcriptome in response to this host-pathogen-diet interaction occurring in situ. The expression of gtfB, and several genes involved in carbohydrate uptake and glycogen metabolism were upregulated, which could modulate the dynamics of biofilm development and pathogenicity [Klein et al., 2009, 2010]. The observations reported here may offer an explanation for the phenomenon that combinations of starch and sucrose are more cariogenic than either alone in animal [Bowen et al., 1980; Firestone et al., 1982] and in situ [Ribeiro et al., 2005] models.
Sparse attention has been devoted to determining the branch structure of polysaccharides found in dental plaque. Earlier examination of pooled plaque samples [Hotz et al., 1972; Emilson et al., 1984] revealed that 18% of plaque is comprised of carbohydrate, the majority of which is water insoluble. Smith degradation showed that α-1,3 or α-1,3/6 are major linkages of the glucan polymer in plaque; some α-1,6-linkage was also detected with smaller amounts of α-1,4-linkages (see role of starch). These observations were in marked contrast to earlier reports which claimed that the dominant polysaccharide in plaque was dextran (with predominantly α-1,6-linked glucose) which is usually highly soluble [Gibbons and Banghart, 1967].
The structure of the polysaccharide in plaque matrix will also be influenced by the duration since the last ingestion of sucrose and starch. Up to 50% of polysaccharide in plaque is metabolized over 4 h at room temperature probably as a result of soluble glucan being digested to glucose and oligosaccharides which are metabolized by bacteria [Critchley et al., 1967; Critchley, 1969; Walker et al., 1981]. Mutanase and dextranase within plaque have the potential to influence the synthesis and structure of glucans. Therefore, a dynamic interaction of the enzymes responsible for glucan synthesis on the one hand with those cleaving the glucosidic linkages (mutanase and dextranase) could be occurring concomitantly in the plaque matrix [Walker et al., 1981; Burne et al., 1986]. It is highly probable that the structure of glucans within plaque matrix undergoes constant change with elevated levels of insoluble polysaccharide in mature plaque [Emilson et al., 1984]. This hypothesis is strongly supported by the observations of Hayacibara et al. , who showed that incorporating dextranase and/or mutanase during the synthesis of glucan by GtfB, C or D in vitro had a profound effect on the amount of glucan formed, its structural properties and bacterial binding sites. Clearly the matrix of plaque is certainly neither static nor homogeneous, but rather undergoing constant restructuring, which can dramatically influence the pathogenicity of this biofilm.
S. mutans harbors 3 distinct gtf genes expressing Gtf activity [Kuramitsu, 1993]. The gtfB (4.4 kbp) and gtfC (4.3 kbp) genes are in an operon-like arrangement and encode GtfB and GtfC enzymes, whereas gtfD gene (5.3 kbp), which is not linked to the gtfBC locus, encodes GtfD enzyme. Overall, GtfB and GtfC are highly homologous sharing about 75% amino acid sequence identity, GtfD a little less so with approximately 50% identity to GtfB and GtfC. The coding sequences of gtfB and gtfC are only 198 bp apart, and can be cotranscribed and be subjected to the same regulatory mechanisms [Ueda et al., 1988; Hudson and Curtiss, 1990; Wexler et al., 1993; Yoshida and Kuramitsu, 2002]. However, it is unclear whether gtfB and gtfC have either a common or an independent promoter. Results from some studies indicate that there is a common promoter upstream of gtfB, which creates a polycistronic message that includes a gtfC coding sequence [Ueda et al., 1988; Hudson and Curtiss, 1990; Wexler et al., 1993; Yoshida and Kuramitsu, 2002], whereas others show a potential independent promoter in the intergenic space [Smorawinska and Kuramitsu, 1995; Fujiwara et al., 1998; Goodman and Gao, 2000]. Nevertheless, the gtfB and gtfC promoters appear to be coordinately expressed [Goodman and Gao, 2000]. On the other hand, gtfD gene is located upstream of gtfBC loci, presents an independent promoter and may be regulated in a manner opposite that of gtfB and gtfC [Wexler et al., 1993; Fujiwara et al., 1998].
There are several factors that can influence the gtf gene transcription, translation and secretion, such as carbohydrate availability/source, environmental pH and growth rate or phase [Wexler et al., 1993; Goodman and Gao, 2000; Li and Burne, 2001; Fujiwara et al., 2002; Abranches et al., 2003; Browngardt et al., 2004; Chen et al., 2006; Shemesh et al., 2006, 2007; Klein et al., 2009]. For example, lowering of the pH following addition of carbohydrates, an increase in the availability of metabolizable carbohydrates sensed via the phosphotransferase system, or production of glycolytic intermediates may regulate the expression of gtf genes. The gtfBC genes are induced in response to acidification or in response to the presence of an excess of a metabolizable carbohydrate (glucose or sucrose) [Li and Burne, 2001]. In addition, inactivation of the gene encoding EIIABman of the phosphotransferase system of S. mutans decreases the gtfBC expression [Abranches et al., 2003]. Results from some studies have shown that sucrose induces the expression of gtfB [Burne et al., 1997; Li and Burne, 2001; Shemesh et al., 2006]. Other investigators reported decreased expression of gtfB and gtfC [Fujiwara et al., 2002]. The transcription and translational expression of gtfD but not gtfB and gtfC appears to be specifically induced by copper ions [Chen et al., 2006]. Few studies evaluated the expression of gtf genes in clinical isolates. Comparison of the gtf genes in clinical isolates revealed that the interstrain difference of gtfB and gtfD was limited, while gtfC showed significant interstrain variations [Fujiwara et al., 1998]. It was also shown that the transcription levels of gtfB and gtfC (and putative transcriptional response regulators) of several clinical isolates of S. mutans (corresponding to distinct genotypes) were growth phase dependent and assumed divergent patterns during specific phases of growth [Stipp et al., 2008]. Recently Klein et al. [2009, 2010] noted that sucrose and starch hydrolysates enhanced the expression of gtfB in S. mutans which resulted in the formation of elevated amounts of insoluble glucans in biofilms formed in vitro, an observation consistent with previous reports [Vacca-Smith et al., 1996a].
RegM (also known as CcpA), the catabolite-repression regulator in S. mutans, appears to be critical for an optimal expression of gtfB and gtfC because inactivation of regM resulted in dramatic decreases in the levels of expression of the gtfBC promoter [Browngardt et al., 2004]. Recently, LuxS-based signaling was shown to be involved in the formation of S. mutans biofilm formation by mediating the expression of gtfB and gtfC, but not the gtfD gene [Yoshida et al., 2006]. The expression of gtfB and gtfC of the S. mutans luxS mutant was enhanced relative to the parental strain whereas the gtfD expression was unaffected. A VicRK signal transduction system in S. mutans also affects gtfBCD expression [Senadheera et al., 2007]; gtfD expression was reduced in the S. mutans vicK null mutant whereas that of gtfB was enhanced when compared to the parent strain [Senadheera et al., 2007]. In particular, deficiency of the trigger factor RopA in S. mutans reduced production of GtfB and GtfD as revealed by Western blotting, but the ropA mutant formed more than 50% more biofilms than the parental strain when sucrose was provided as the supplemental carbohydrate source [Wen et al., 2005]. Clearly, the mechanisms involved in the regulation of the genes encoding Gtf enzymes appear to be complex and still remain to be fully explored. Nevertheless, it is noteworthy that the expression of Gtfs in S. mutans is greatly enhanced when the organisms are grown within a biofilm [Burne et al., 1997]. Much of the work reported above was conducted in vitro; nevertheless, it is clear that comparable conditions could readily arise in plaque formed in vivo.
Role of Each Gtf in Dental Caries Pathogenesis
There are well-defined hypotheses for the role of each Gtf in the pathogenesis of dental caries. Because each enzyme has properties in common (e.g. binding to sHA), it is unclear whether all these enzymes are essential for the complete expression of virulence. Using an in vitro model, Ooshima et al.  and Tamesada et al.  showed that the presence of GtfC enhanced the amount of glucan formed. In contrast, van der Ploeg and Guggenheim  and Thurnheer et al. [2003, 2006] claimed that deletion of GtfC from S. mutans in their multispecies biofilm model was without effect on the matrix of the biofilm but did affect the physical properties of the glucan, an observation consistent with the demonstrated effects of antibody on the structure of glucan [Wunder and Bowen, 2000; Kopec et al., 2002]. A mutant S. mutans that harbored only GtfC was significantly (76%) less cariogenic than the parent strain that contained the full complement of gtf genes [Wunder and Bowen, unpubl.]. We suggest that GtfC is adsorbed into pellicle where – when exposed to sucrose – it forms glucan in situ; however; it is clear that GtfB may also bind to sHA but with less avidity. The glucans formed on the surface provide an initial matrix that holds bacterial cells together on the sHA surface [Vacca-Smith and Bowen, 1998, 2000; Koo et al., 2010b].
GtfB in contrast binds to many oral microorganisms and in the presence of sucrose and starch hydrolysates forms an insoluble, structurally rigid and cohesive matrix for plaque biofilm [Koo et al., 2010b]; GtfB appears to be responsible for the development of highly structured microcolonies by S. mutans either alone or in the presence of other organisms [Koo et al., 2010b; Xiao and Koo, 2010]. GtfD forms soluble glucans that serve as a primer for GtfB and also as a reserve polysaccharide that can be metabolized by plaque bacteria [Critchley et al., 1967; Walker et al., 1981]. It is highly likely that other soluble glucans from oral microorganisms could also serve as primers for GtfB [Kuramitsu, 1974; Hamada and Torii, 1980; Koga et al., 1983; Tamesada et al., 2004; Reese and Guggenheim, 2007]. However, the effects of soluble glucan primer on the insoluble glucan synthesis are variable depending on the concentration of the dextrans; glucan synthesis was enhanced by low concentrations (1– 5 mg/ml) of water-soluble dextrans of various molecular weights, but higher concentrations (10 mg/ml) inhibited glucan synthesis [Hamada and Torii, 1980]. Therefore, it is tempting to speculate that formation and subsequent structure of glucans are influenced by the availability and the structure of the primer glucan which is usually soluble. The interaction of Gtf enzymes responsible for the synthesis of insoluble and soluble EPS may be critical for the optimal biofilm accumulation by S. mutans within a multispecies system [Tamesada et al., 2004; Koo et al., 2010b].
Overall, all Gtfs from S. mutans appear to play an important role in the formation of virulent plaque via production of a variety of glucans with distinct function and structure. Our observations support previous findings indicating the critical role of S. mutans Gtfs and their products in the pathogenesis of dental caries [Tanzer et al., 1974; Yamashita et al., 1993; Mattos-Granner et al., 2000; Vacca-Smith et al., 2007].
Inhibition of Gtfs
Following recognition of the importance of Gtf in the pathogenesis of dental caries, specific inhibition of Gtfs as a means to prevent plaque-related diseases became attractive. Such a selective approach on a proven virulence property intuitively appears more attractive than using a nonspecific antimicrobial agent. Furthermore, it is critical to note that agents which inhibit Gtf in solution may be without effect when the enzyme is adsorbed to a surface [Vacca-Smith and Bowen, 1996; Wunder and Bowen, 1999; Koo et al., 2002c]. Gtf has at least 2 subsites, glucosyl and fructosyl, that could be targets for inhibitors [Devulapalle and Mooser, 2000]. The site containing 3 aspartic acid residues has been identified as the location for glucose conjugation. Zn2+ has been shown to bind to the fructose site. In addition, the enzyme has several separate glucan-binding sites including one found on a 60-kD domain at the C terminus [Mooser and Wong, 1988]. Clearly there are additional sites on Gtfs to which potential inhibitors could bind.
Although it is recognized that agents which inhibit enzymes in solution may be without effect when the enzymes are adsorbed to a surface [Scheie and Kjeilen, 1987; Vacca-Smith and Bowen, 1996b; Wunder and Bowen, 1999], in general, it has been observed that inhibitors which bind to an active site in solution have a similar effect when the enzyme is bound to a surface. Examples would include deoxynojirimycin, tris(hydroxymethyl)aminomethane and trichlorogalactosucrose [Devulapalle and Mooser, 1994; Wunder and Bowen, 1999; Wright et al., 2002]. They probably bind to the aspartic acids in the active site and act by blocking the formation of glucose transition molecules.
Results from early work revealed that a diverse range of compounds, such as quaternary ammonium compounds, aliphatic amines and antibodies, were effective in inhibiting to a greater or lesser degree undetermined mixtures of Gtfs in solution [Ciardi et al., 1978]. In addition, many natural agents have been explored for their effect on Gtf activity, such as hops, green tea, traditional medicinal plants and food extracts [Wu-Yuan et al., 1988; Ikeno et al., 1991; Otake et al., 1991; Nakahara et al., 1993; Wolinsky et al., 1996; Tagashira et al., 1997; Osawa et al., 2001; Steinberg et al., 2004; Furiga et al., 2008; Hannig et al., 2008b; Yaegaki et al., 2008]. Carbohydrate fatty esters had no effect on Gtf activity from S. sobrinus despite inhibiting growth of the organisms [Devulapalle et al., 2004]. In contrast, oleanic and oleic acid were efficient inhibitors of Gtf activity in solution [Kozai et al., 1987; Won et al., 2007]; the number of double bonds present along with free carboxyl groups was associated with inhibitory activity. According to Yanagida et al. , the high-molecular-weight plant polyphenols displaying strong anti-Gtf activity have a common structural feature shared with catechin-based oligomeric forms (condensed tannins) and/or gallate ester form compounds (hydrolyzable tannins). However, data from studies using mixtures of Gtfs are difficult to interpret because a specific enzyme might be inhibited and the other enzymes in this mixture enhanced, and furthermore the assays were conducted in solution phase. Several substances, many of which are found in plaque, were identified which enhanced activity, e.g. cardiolipin, putrescine and cadaverine [Ciardi et al., 1978].
A large number of compounds have been examined by our laboratory using individual purified Gtfs (B, C and D enzymes) both in solution phase and adsorbed to sHA surface, including perborate, sodium, metaperiodate, metal ions and naturally occurring substances [Vacca-Smith and Bowen, 1996; Wunder and Bowen, 1999; Koo et al., 2000, 2002c]. Among them, metal ions Fe2+Zn2+Cu2+ and some oxidizing agents (hypochlorite and rose Bengal) exhibited inhibitory properties, which were usually greater when the enzymes were in the soluble phase [Wunder and Bowen, 1999]. Metal ions probably exert their inhibiting effects through the Fenton reaction where they combine with peroxide to produce hydroxyl radical ions [Devulapalle and Mooser, 2001]. Copper ions have also been shown to depress the expression of gtf genes selectively [Chen et al., 2006].
A range of ingredients commonly found in over-the-counter oral hygiene products have been examined for their effects on the 3 common Gtfs in solution and on a surface [Vacca-Smith and Bowen, 1996]. The activity of GtfB in solution was greatly reduced by many commercially available agents, e.g. cetylpyridinium chloride, alexidine dihydrochloride or triclosan; these same agents had a reduced inhibiting effect on enzyme activity adsorbed to a surface. Remarkably few agents had any effect on GtfC with the exception of chlorhexidine which reduced the activity of the enzyme in solution by more than 60%. GtfC has many hydrophobic domains particularly at the C terminus [Ueda et al., 1988] and may block access by hydrophilic inhibitors to the active site which may explain its comparative resistance to inhibitory agents. Overall it is apparent that the 3 Gtfs are unequally affected by commercial antiplaque agents [Vacca-Smith and Bowen, 1996; Wunder and Bowen, 1999].
Inhibitory effects of several naturally occurring products such as propolis, plants, cranberry extracts and their constituents have been examined as well [Koo et al., 2000, 2002c, 2006, 2010a, b; Gregoire et al., 2007; Murata et al., 2008]. Many of them display partial inhibition of GtfB and GtfC in solution, but only few are potent inhibitors (>90% inhibition) and even fewer disrupt the activity of surface-adsorbed enzymes. Aqueous-ethanol extracts of propolis (a resinous substance collected by honeybees from various parts of plants) were particularly effective inhibitors of GtfB and GtfC both in solution and on the surface [Koo et al., 2000]. However, the bioactivity of propolis was variable depending on the geographic origin and the biodiversity of the region of sample collection, which influences the chemical composition of this natural product [Koo et al., 1999, 2000]. Further investigation identified specific low-molecular-weight flavones and flavonols as the primary compounds in propolis responsible for inhibition of Gtf activity [Koo et al., 2002c]. Among them, apigenin (4’,5,7-trihydroxyflavone) was a highly effective inhibitor of Gtfs (noncompetitive inhibition) even at micromolar concentrations. The presence of hydroxyl (OH) groups at specific positions and the double bond between C2 and C3 in the molecular structure of apigenin may provide a site for nucleophilic addition by side chains of amino acid in Gtfs, which could disrupt the enzymatic activity [Koo et al., 2002b]. It is noteworthy that apigenin also decreased the expression of gtfB and gtfC by planktonic cells and biofilms of S. mutans without affecting the bacterial viability [Koo et al., 2006].
Recently, specific high-molecular-weight A-type proanthocyanidin oligomers (dimers to dodecamers) isolated from aqueous extract of cranberry effectively diminished the synthesis of insoluble glucans by surface-adsorbed GtfB [Koo et al., 2010a]. The high-molecular- weight polyphenols may have site-specific actions as reported by Matsumoto et al. , who demonstrated that the oolong tea fraction rich in polymeric polyphenols reduced glucan synthesis noncompetitively by targeting the glucan-binding domain of S. mutans GtfB and GtfD in solution phase. The high-molecular-weight polymeric proanthocyanidins consisting exclusively of epicatechin units linked mainly by C-4β and C-8 bonds were identified as major bioactive agents in cocoa extracts [Osawa et al., 2001]. We found that the presence of A-type double interflavan linkage (which confers structural rigidity to the molecule) and a degree of polymerization ranging from 4 to 12 were considered optimal for effective inhibition of surface-adsorbed enzyme [Koo et al., 2010a]. The actions on Gtfs, especially surface-adsorbed GtfB and GtfC, were found to be one of the major mechanisms by which topical application of A-type proanthocyanidins effectively reduces biofilm accumulation on apatitic surfaces in vitro, and development of dental caries in vivo without displaying microbiocidal activity [Koo et al., 1999, 2002a, b, 2003, 2005, 2010a]. Nevertheless, the exact mechanisms of Gtf inhibition by these bioactive naturally occurring agents remain to be elucidated.
The possibility of developing an effective vaccine against dental caries has attracted considerable attention over many years [Taubman and Nash, 2006]. Gtfs and fragments of the molecules have been used as an immunogenic agent [Culshaw et al., 2007].
This part of our review focuses on using antibodies that inhibit one or more Gtfs as topical agents. The effects of specific antibodies on the activity of Gtfs and structure of the product glucan have received some attention [Kuramitsu and Ingersoll, 1978b; Kopec et al., 2002]. Interpretation of earlier data is often difficult because in many instances, nondetermined mixtures of Gtfs have been used in the assay or in the preparation of antibodies. Further complications arise from the observation that normal serum harbors substances that enhance Gtf activity [Schachtele and Harlander, 1983]. As a consequence, data on the effect of antibody on Gtf sometimes reported as inhibition is in fact merely a reduction in enhancement; the net effect of the antibody may be enhancement of glucan production [Ciardi et al., 1978; Oho et al., 1999; Kopec et al., 2002]. There are numerous reports on the influence of various antibody preparations on in vitro phenomena such as cell aggregation, glucan synthesis and adhesion to glass surfaces [Olson et al., 1974; Douglas and Russell, 1982; Oho et al., 1999; Kawato et al., 2008]. Few studies appear to have explored the effects of antibodies to specific Gtfs in solution or on a surface, and structure of glucans [Wunder and Bowen, 2000; Kopec et al., 2002]. The structure of GtfB and GtfC glucans formed in the presence of antiserum differed from that of controls based on the glucan susceptibilities to dextranase and mutanase and linkage analyses.
Antibodies to various preparations of Gtf have been raised in bovines, hens and used topically to determine their effects on caries in animals and on activity in vitro [Hamada et al., 1991; Krüger et al., 2004]. Topical application of egg-derived antibody that inhibited GtfB (insoluble glucan production) had a dramatic effect on the incidence of caries in rats compared with controls [Hamada et al., 1991; Krüger et al., 2004]. Antibody to the enzyme synthesizing soluble glucan was without effect. These observations are supportive of the importance of GtfB in the pathogenesis of dental caries. Topical application of antibodies to hybrid GtfB and proanthocyanidin (saliva-binding protein) reduced the incidence of caries in rats [Mitoma et al., 2002]. It was also noted that antibodies effective against GtfB and GtfC in solution had significantly less effect when the enzymes were adsorbed to a surface which suggests that the antibody was not directed against the active site. Antibodies to GtfD were without effect on the activity of GtfB or GtfC [Kuramitsu and Ingersoll, 1978b].
Use of topical antibodies to affect plaque formation has some attraction because the target of action can be highly specific. Furthermore, additional therapeutic agents could be attached to the antibody molecule and thereby lead to the development of a highly selective delivery system.
Conclusions and Future Insights
Gtfs play an essential role in the expression of virulence by S. mutans in animal models. Free Gtf is incorporated in an active form into tooth pellicle, and the adsorbed enzyme displays enhanced activity over a wide range of pH values compared with the same enzyme in solution. Exposure of the adsorbed enzyme to sucrose or a combination of sucrose and starch results in formation of glucan in situ which provides binding sites for a diversity of microorganisms. Gtfs readily adsorb, even in the presence of saliva, to a wide range of bacteria, thereby converting them into de facto glucan producers. These biological events (fig. 2) probably explain the images of bacteria observed within plaque surrounded by a polysaccharide matrix. Gene expression of GtfB and GtfC is upregulated when S. mutans is grown on a surface and in response to acidification of the environment. Thus, Gtfs can perform even under the most extreme conditions experienced in the mouth.
The structure and 3-dimensional architecture of the polysaccharide matrix probably changes over time as a result of environmental challenges found in the oral cavity, such as the action of mutanase and dextranase found within plaque. Gtf being a primary virulence property of S. mutans appears to offer a major and selective target for chemotherapeutic agents to prevent the formation of cariogenic plaque. A large number of agents have been identified that inhibit Gtfs in solution but have a reduced or no effect on adsorbed enzymes. Metal ions, sugar analogs, lipids, natural products and antibodies have been explored for inhibitory effects.
It is clear that Gtfs acting in concert play a critical role in the formation of plaque and in the pathogenesis of dental caries. It is equally apparent that the behavior of these enzymes in solution does not mirror that observed when the enzyme is adsorbed to a surface. The conformational changes associated with the adsorption of salivary and microbe-derived proteins to surfaces are critical to understanding the initiation and subsequent accumulation of biofilms. In addition, results from such investigations are likely to lead to acquiring agents that have enhanced power to inhibit Gtfs in all phases.
Clearly, the reactions of Gtfs in pellicle and in plaque are diverse and complex and remain a challenging enigma. Exploration of the dynamics of the microenvironments within plaque using in situ models in real time could enhance our understanding of the biological phenomena and physical changes within dental plaque. The results of such investigations may have import well beyond the mouth.
The authors’ research in this area was supported by grants from the National Institute for Dental and Craniofacial Research (NIDCR/NIH P01 DE11549 and R21 DE15564, to W.H.B.; R01 DE16139 and DE18023, to H.K.). The authors also thank Dr. Jin Xiao for acquiring and processing the confocal fluorescence images of the biofilms.
William H. Bowen, BDS, PhD
University of Rochester, Center for Oral Biology
601 Elmwood Avenue, Box 611
Rochester, NY 14642 (USA)
Tel. +1 585 275 0772, E-Mail William_Bowen@urmc.rochester.edu
Received: May 26, 2009
Accepted after revision: January 26, 2011
Published online: February 23, 2011
Number of Print Pages : 18
Number of Figures : 2, Number of Tables : 0, Number of References : 187
Vol. 45, No. 1, Year 2011 (Cover Date: April 2011)
Journal Editor: Beighton D. (London)
ISSN: 0008-6568 (Print), eISSN: 1421-976X (Online)
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