Bacterial Biofilm Eradication Agents: A Current Review
- 1Institute of Health and Biomedical Innovation, Queensland University of Technology, Brisbane, QLD, Australia
- 2School of Biomedical Sciences, Queensland University of Technology, Brisbane, QLD, Australia
- 3School of Chemistry, Physics, and Mechanical Engineering, Queensland University of Technology, Brisbane, QLD, Australia
Most free-living bacteria can attach to surfaces and aggregate to grow into multicellular communities encased in extracellular polymeric substances called biofilms. Biofilms are recalcitrant to antibiotic therapy and a major cause of persistent and recurrent infections by clinically important pathogens worldwide (e.g., Pseudomonas aeruginosa, Escherichia coli, and Staphylococcus aureus). Currently, most biofilm remediation strategies involve the development of biofilm-inhibition agents, aimed at preventing the early stages of biofilm formation, or biofilm-dispersal agents, aimed at disrupting the biofilm cell community. While both strategies offer some clinical promise, neither represents a direct treatment and eradication strategy for established biofilms. Consequently, the discovery and development of biofilm eradication agents as comprehensive, stand-alone biofilm treatment options has become a fundamental area of research. Here we review our current understanding of biofilm antibiotic tolerance mechanisms and provide an overview of biofilm remediation strategies, focusing primarily on the most promising biofilm eradication agents and approaches. Many of these offer exciting prospects for the future of biofilm therapeutics for a large number of infections that are currently refractory to conventional antibiotics.
Biofilm formation is a significant virulence mechanism in the pathogenesis of many medically important bacterial pathogens, such as Pseudomonas aeruginosa (Gellatly and Hancock, 2013), Staphylococcus aureus (Gordon and Lowy, 2008), and Escherichia coli (Beloin et al., 2008). The number of diseases being attributed or associated with biofilm infections is large, with some common examples including vaginitis (Machado et al., 2016), colitis (von Rosenvinge et al., 2013), conjunctivitis (Behlau and Gilmore, 2008), gingivitis (Vieira Colombo et al., 2016), urethritis (Delcaru et al., 2016), and otitis (Post, 2001). In fact, it is estimated that ~80% of all microbial infections in humans are a direct result of biofilms (Davies, 2003). One biofilm-related infection of particular medical concern is P. aeruginosa biofilms in the lungs of cystic fibrosis patients. This opportunistic pathogen has been known to cause acute and chronic lung infections that can result in significant morbidity and mortality (Wagner and Iglewski, 2008). A second area of considerable concern is that of chronic wound infections. Highly persistent biofilm-related wound infections, which commonly involve the pathogens P. aeruginosa and S. aureus (Omar et al., 2017), are suggested to be responsible for over 80% of the 100,000 limb amputations carried out on diabetic patients in each year (James et al., 2008). An additional area of importance when considering biofilm-related infection is implanted medical devices. Microbial adhesion resulting in biofilm formation on implanted medical devices is a common occurrence and can lead to serious illness and death (Habash and Reid, 1999). These implanted medical devices, which can include intravascular catheters, urinary catheters, pacemakers, heart valves, stents, and orthopedic implants, are commonly used to saves lives but can present a significant health risk when colonized by bacterial biofilms (Francolini and Donelli, 2010).
Most antimicrobial treatments available are generally developed and evaluated against microorganisms in the planktonic (free-living) mode of life. Consequently, these treatments are often ineffective against pathogenic biofilms (Costerton et al., 1987; Lebeaux et al., 2014), which can be up to one thousand times more tolerant to antimicrobial treatments (Stewart and William Costerton, 2001; Luppens et al., 2002; Davies, 2003). The phenomenon of biofilm recalcitrance makes them extremely difficult to treat and eradicate effectively. Thus, new strategies for the prevention, dispersal and treatment of bacterial biofilms are urgently required. This review presents an overview of bacterial biofilm development and the current methods used to prevent, disperse, and treat bacterial biofilms, with a particular focus on the development of novel biofilm eradication strategies.
Biofilms are complex three-dimensional communities of microorganisms adhering to a surface and encased in a protective exopolymeric substance. Biofilm formation progresses over five main stages (Figure 1). In stage one, individual planktonic cells migrate and adhere to a surface. Providing the correct conditions are present, these adherent cells then initiate biofilm production on the surface and become encased in small quantities of exopolymeric material. In stage two, adherent cells exude an extracellular polymeric substance (EPS) and become irreversibly attached to the surface, which results in cell aggregation and matrix formation. In stage three, the biofilm begins to mature by developing microcolonies and water channel architecture, while also becoming significantly more layered. In stage four, the fully mature biofilm reaches its maximum cell density and is now considered a three-dimensional community. In stage five, the mature biofilm releases microcolonies of cells from the main community, which are free to migrate to new surfaces spreading the infection to other locations (Stoodley et al., 2002; Schachter, 2003).
Figure 1. A model showing the typical stage-wise development of a bacterial biofilm accompanied by transmitted light microscopy images showing these different stages for a P. aeruginosa biofilm. Republished with permission of Annual Reviews, Inc. (Stoodley et al., 2002); permission conveyed through Copyright Clearance Center, Inc.
The Extracellular Polymeric Substance (EPS)
The extracellular matrix encasing the cells in a biofilm, also referred to as the EPS, is composed of a complex mixture of proteins, lipids, nucleic acids (extracellular-DNA), and polysaccharides (Annous et al., 2009). These constituents not only assist in securing the biofilm to the surface, but also trap nutrients, provide structural support, and shield against host immune responses and antimicrobial treatments (Flemming et al., 2007). In addition to the above functions, the EPS is also responsible for holding the community of biofilm cells in close proximity, thereby enabling cell-to-cell communication (quorum sensing), and facilitating the exchange of genetic material through horizontal gene transfer (Hausner and Wuertz, 1999).
Cell-to-cell Communication (Quorum Sensing)
Biofilms are known to control their population density through a cell-to-cell signaling mechanism known as quorum sensing (Schachter, 2003). Cell-to-cell communication is a complex regulatory process which prevents biofilm cell density from reaching an unsustainable level (Nadell et al., 2008). Quorum sensing is reliant on signaling molecules known as autoinducers (Figure 2). These autoinducers are constantly being produced by the bacterial cells, and thus, as cell density increases, so does the level of autoinducers (Figure 3). At a specific cell density, a critical threshold concentration of autoinducers is reached, which is known as the quorum level (Annous et al., 2009). During this time, autoinducer receptor binding leads to the repression or activation of several target genes. This modulation of the quorum sensing process allows bacteria to display a unified response that benefits the entire bacterial community by maintaining the optimal biofilm size and co-ordinating virulence phenotypes (Nadell et al., 2008; Annous et al., 2009; Dickschat, 2010). This unified response allows the biofilm to behave more like a multicellular organism, which enables the bacterial community to adapt to changing environmental conditions. The benefit of quorum sensing is not limited to controlling population density. In fact, quorum sensing has also been shown to aid the spread of beneficial mutations throughout the biofilm colony, enhance access to nutrients, and contribute to antibiotic tolerance (Hannan et al., 2010).
Figure 2. Chemical structure of two predominant types of small molecule autoinducers involved in quorum sensing.
Figure 3. Quorum sensing illustration. During planktonic cell growth (blue ovals), the relative amount of autoinducers (red triangles) is proportionally low. As cells enter a densely populated mode of growth (green ovals) the relative proportion of autoinducers increases.
Biofilm Antibiotic Tolerance (BAT)
Bacteria in biofilms are inherently more tolerant to antimicrobial treatment when compared directly to planktonic cells of the same strain. In fact, studies have shown that bacteria growing in biofilms are often thousands of times more tolerant to antimicrobial treatment than their planktonic counterparts (Stewart and William Costerton, 2001; Luppens et al., 2002; Davies, 2003). While, the mechanisms of antibiotic resistance in planktonic bacteria are generally well-understood (Munita and Arias, 2016), those same mechanisms (mutations, efflux pumps, and antibiotic modifying enzymes) do not appear to be the main cause of biofilm-mediated antibiotic tolerance. For example, inherently drug-susceptible bacterial strains often exhibit significant antibiotic tolerance when in the biofilm mode of life, however, when biofilm-residing cells are dispersed (released) from the main community, antimicrobial susceptibility is quickly restored for these cells (Anderl et al., 2000). Thus, biofilm antibiotic tolerance (BAT) is thought to involve alternative mechanisms to bacterial antimicrobial resistance.
BAT has been defined as the ability of biofilm-residing bacteria to survive antimicrobial treatment by utilizing their existing complement of genes (Anderson and O'Toole, 2008). BAT can be grouped into two categories: innate (resulting from growth in a biofilm) and induced (resulting as a response to antimicrobial treatment). Several major innate factors have been identified which directly influence BAT (Costerton et al., 1999; Lewis, 2001; Donlan and Costerton, 2002; Dunne, 2002; Stewart, 2002; Hoiby et al., 2010) and are briefly discussed below (Figure 4).
Figure 4. Proposed mechanisms contributing to biofilm antimicrobial tolerance (BAT). The biofilm shown is comprised of bacteria (circles and ovals), which are encapsulated by the extracellular polymeric substance (EPS) (dark-brown line surrounding biofilm and multi-colored background within biofilm). Red stars represent antibiotics which are in contact with the biofilm. Restricted penetration of antibiotics through the biofilm EPS is depicted by the black arrows (indicating antibiotics failing to penetrate the EPS of the biofilm) and the red stars at the surface of the biofilm (indicating antibiotics that have failed to diffuse past surface-residing cells). Orange circles and ovals surrounded with yellow/tan background represent surface-residing cells which are in contact with the antibiotics (red stars). Green circles and ovals surrounded by a blue/gray background are indicative of microenvironments within the biofilm (areas of reduced oxygen concentration and reduced cell replication). Purple circles indicate persister cells present within the biofilm (small subpopulation of cells within the biofilm that enter a protected metabolically quiescent state recalcitrant to the action of antimicrobials). Image adapted from Penesyan et al. (2015).
Innate Factors Mediating BAT
The EPS of a biofilm has long been considered the major contributor to BAT (Donlan and Costerton, 2002). However, the supporting evidence for this is conflicting. The EPS of several biofilm-forming species have demonstrated an innate ability to prevent antibiotic penetration (Campanac et al., 2002; Davenport et al., 2014). However, this phenomenon is not conserved between the EPS of all biofilm-forming species and also appears to be antibiotic specific. For example, ciprofloxacin and ampicillin were found to effectively penetrate and diffuse through Klebsiella pneumoniae biofilms, ultimately reaching distal cells (Anderl et al., 2000). Furthermore, ciprofloxacin also exhibited similar penetration and diffusion activity in P. aeruginosa biofilms (Walters et al., 2003). Likewise, tetracycline was able to effectively reach all cells within E. coli biofilms (Stone et al., 2002). Interestingly, many of these antibiotics are still ineffective at eradicating the biofilm. While restricted penetration may be a major contributing factor of BAT for some antibiotics in some biofilms, its effects are certainly not universal. Thus, additional or complementary mechanisms that facilitate BAT also exist.
Reduced Growth Rate
While restricted pentation does not always explain BAT, reduced growth rate appears to play a far more evident role in BAT. The complex internal structure of a biofilm is known to produce microenvironments, which are deprived of oxygen and nutrients (Brown et al., 1988). Deprivation of oxygen and nutrients are well-established cues for slowed bacterial growth and antimicrobial resistance in many species (Brown et al., 1988; Field et al., 2005). Considering most antibiotics target rapidly replicating bacterial cells, it is of little surprise that areas of slow-growing or dormant cells within a biofilm would be unaffected by antibiotics and thus exhibit high levels of antibiotic tolerance. Several studies have demonstrated a direct link between biofilm microenvironments, which produce slow-growing cells and BAT (Anderl et al., 2003; Walters et al., 2003; Borriello et al., 2004). However, not all antimicrobial agents require rapidly replicating cells to facilitate their mode of action, and many of these agents are still highly tolerated by biofilms, for example, chlorine in the treatment of multi-species biofilms (Barraud et al., 2009). Thus, slow bacterial growth alone is not sufficient to confer BAT either.
Persister cells represent a minute subpopulation of bacterial cells, which exist in a dormant state and exhibit extreme antimicrobial tolerance (Wood et al., 2013). The presence of persister cells within a bacterial population is not a recent discovery; in fact, their existence was first described as early as 1942 (Hobby et al., 1942). Early studies discovered that when a planktonic population of S. aureus cells was treated with penicillin, ~1% of the cells were not killed. Two years later, Bigger supported this finding and documented that one out of a million S. aureus cells was not killed by treatment with penicillin (Bigger, 1944). Furthermore, Bigger also determined that these surviving cells, which he termed persisters to differentiate them from resistant mutants, had not undergone a genetic alteration, but instead were simply a phenotypic variant that was tolerant to antibiotics. Despite their early discovery, the role of persister cells in bacterial pathogenesis remained largely unexplored until the study of bacterial biofilms uncovered the significant role of persister cells in BAT (Lewis, 2010).
Unlike planktonic bacterial populations the presence of persister cells within a biofilm community affords them protection from elimination by the immune system, and despite their small numbers, their contribution to pathogenesis becomes more significant in biofilm infections (Lewis, 2005, 2010). Several studies have now demonstrated that after treating a biofilm with antibiotics, a small population of persister cells will remain regardless of the concentration of antibiotic utilized (Spoering and Lewis, 2001; Harrison et al., 2005a,b). Once the treatment ceases and the antibiotic concentration decreases, these remaining persister cells can act as a nucleation point to repopulate the biofilm, ultimately producing a relapsing biofilm infection (Lewis, 2001). Interestingly, the majority of these repopulated biofilm residing cells exhibit no additional antimicrobial tolerance or resistance compared to the original cells that were eradicated, strongly supporting that the persister state is a phenotypic variant rather than a mutation.
The universal presence of persister cells within biofilms is perhaps the most plausible innate mechanism of BAT described so far, and while persisters do not harbor antimicrobial resistance genes directly, they certainly provide a perfect platform for the development of resistant mutants. Consequently, many research groups have focused their efforts on investigating the mechanisms of persister cell formation (Keren et al., 2004a,b; Spoering et al., 2006), with the hope that their findings will enable the development of antibacterial agents which can target and eradicate these fascinating cells.
Induced BAT Mechanisms
The mechanisms of induced BAT appear to be more complicated than the innate factors contributing to this phenomenon and are less well-understood with only a few studies on the topic (Bagge et al., 2004a,b; Szomolay et al., 2005; Redelman et al., 2014; Zhao et al., 2015). Antimicrobial treatment represents a significant stress signal for biofilm-residing cells, and consequently, it is reasonable to assume that antimicrobial treatment could select biofilm-specific antimicrobial resistance genes, and these genes would contribute to BAT. An interesting example of how antibiotics can induce such a response in biofilms is the effect that some antibiotics have on EPS production. Ziebuhr et al. documented how administering sub-inhibitory concentrations of several common antibiotics to Staphylococcus epidermidis biofilms activated the expression of the ica gene cluster, which mediates the production of polysaccharide intercellular adhesin (PIA), a vital factor for S. epidermidis biofilm formation (Rachid et al., 2000). Young et al. and Hoiby et al. found similar effects, albeit with different genes in E. coli and P. aeruginosa, respectively (Sailer et al., 2003; Bagge et al., 2004b). While these examples have not specifically been linked to BAT the idea that biofilm residing bacteria may regulate the expression of specific genes in response to antimicrobials to facilitate BAT certainly appears plausible.
Biofilm Inhibition Strategies
The material matrix of implanted medical devices and biomaterials provide an ideal site for bacterial adhesion promoting mature biofilm formation (Arciola et al., 2012). Thus, methods which prevent bacterial attachment to these materials represent an obvious preventative strategy. The most common method for preventing bacterial adhesion is surface modification. Here, the exterior surface of the implanted medical device or biomaterial is altered, either directly or with the aid of a coating, to produce a barrier which is inhospitable to bacteria (Bazaka et al., 2012). This strategy has shown significant promise for preventing biofilm-related infections resulting from orthopedic implants (Arciola et al., 2012). Thus, the area of surface modification to prevent biofilm formation is a large field, and many comprehensive reviews on this topic already exist (Katsikogianni and Missirlis, 2004; Arciola et al., 2012; Bazaka et al., 2012; Campoccia et al., 2013).
The use of small molecule biofilm inhibitors is another approach used to prevent biofilm formation. In fact, the anti-biofilm properties of a biofilm inhibitor are often employed to passivate the surface of an implanted medical device or biomaterial (Nablo et al., 2005; Boase et al., 2018). The use of biofilm inhibitors is one of the largest areas in biofilm remediation research with a plethora of unique biofilm inhibitors currently described (e.g., phenols, imidazoles, furanone, indole, bromopyrrole, etc.) (Rabin et al., 2015). As such, there are many comprehensive reviews on the topic of biofilm inhibition agents (Simões et al., 2010; Worthington et al., 2012; Rabin et al., 2015).
Biofilm Dispersal as a Treatment Strategy
Biofilm dispersal agents generally interfere with chemical pathways or processes, such as quorum sensing, which are required for bacteria to maintain the biofilm mode of existence (McDougald et al., 2012). As disperser cells are generally more susceptible to antimicrobial treatment than biofilm-residing cells, this strategy has recently become an intense area of study. Consequently, a variety of new and promising biofilm dispersal agents have been discovered and reviewed by others (Fleming and Rumbaugh, 2017; Guilhen et al., 2017; Roy et al., 2018). While promising, the use of biofilm-dispersal agents as a treatment strategy can be problematic, as disperser cells, if left untreated, are likely to translocate and seed infection in new areas, ultimately spreading the initial infection. Hence, most dispersal agents are utilized as a combined treatment where the dispersal agent is co-administered with an antimicrobial agent (Marvasi et al., 2014; Reffuveille et al., 2015). Co-treatment generally involves administering a combination of drugs concurrently, in this case, a biofilm dispersal agent and an antibiotic, to exert a synergistic effect. While co-administering a dispersal agent with an antibiotic has yielded some promising results in vitro (Barraud et al., 2006; Reffuveille et al., 2015; Roizman et al., 2017), this treatment strategy can be challenging to translate in the clinic, as ensuring that both agents are present at the target site in the correct concentration is often difficult (Fleming and Rumbaugh, 2018). Furthermore, drug co-administration treatments are often associated with several challenges, including complex treatment schedules, increased risk of adverse effects, increased treatment costs, and antagonism (Rybak and McGrath, 1996; Tamma et al., 2012). Consequently, standalone treatments, such as the development of biofilm eradication agents (BEAs) have become an attractive option.
Biofilm Eradication Agents
BEAs are antibiotics which can target and eradicate biofilm-residing cells as a standalone treatment. The design and discovery of BEAs constitute an emerging area in biofilm remediation research. A variety of promising BEAs have already been developed, and their activity, design, and potential uses are reviewed below.
Antimicrobial peptides (AMPs) are one of the most well-studied classes of BEAs and are often considered an attractive alternative to antibiotics (Baltzer and Brown, 2011). They are ubiquitous compounds, produced in a variety of plant, invertebrate, and animal species. AMPs can vary greatly in size (between five to over ninety amino acids) and molecular mass (between 1 and 5 kDa). They are most commonly cationic in nature (overall positive charge), which has led to them being referred to as cationic antimicrobial peptides (Brown and Hancock, 2006); however, anionic forms have also been reported (Harris et al., 2009). Their antimicrobial mechanism of action is still not fully understood, but their activity is often linked to cytoplasmic membrane disruption and inhibition of protein folding or enzyme activity (Shai, 1999; Bechinger and Gorr, 2017). While the potential use of AMPs as an alternative to antibiotics has received a great deal of attention over the past several decades, their use against microbial biofilms is far most recent.
LL-37 (Figure 5) was one of the first AMPs reported as possessing the potential for biofilm eradication (Overhage et al., 2008). LL-37 is a human cathelicidin-derived broad spectrum AMP, which is amphipathic and found in most bodily fluids (Burton and Steel, 2009; Nijnik and Hancock, 2009). Hancock first reported that low concentrations (0.11 μM) of LL-37 were able to decrease P. aeruginosa cell attachment to plastic surfaces, while higher concentrations (0.9 μM) reduced the overall thickness of established biofilms (40% reduction in thickness) (Overhage et al., 2008). In a subsequent study by Cohen, LL-37 was found to eradicate P. aeruginosa biofilms in an in vivo animal model at a concentration of 556 μM (Chennupati et al., 2009). Interestingly, in a separate study by Marchini, LL-37 was also shown to exhibit anti-biofilm activity against the Gram-positive pathogen Staphylococcus epidermidis with low concentrations (0.22 μM) preventing cell attachment and higher concentrations (0.22–7.12 μM) preventing mature biofilm establishment (Hell et al., 2010). While the study did not directly examine S. epidermidis biofilm eradication by LL-37, similarities in its biofilm inhibition concentrations with P. aeruginosa would suggest that its eradication activity is likely to be broad-spectrum. In a more recent study by Li and co-works, LL-37 was found to exhibit potent S. aureus biofilm eradication activity (Kang et al., 2019). LL-37 was able to significantly eradicate S. aureus biofilm residing cells (>4-log reduction in CFU) (Kang et al., 2019). LL-37 certainly appears to exhibit many of the characteristics of a promising BEA, it has both Gram-negative and Gram-positive efficacy, and low human cell toxicity (Gordon et al., 2005), however, its use as a BEA remains limited. Instead, LL-37 seems to function better as a biofilm inhibitor (Overhage et al., 2008) rather than a true BEA. Nevertheless, the potential of this AMP has undoubtedly been demonstrated, and hopefully investigations into its use as a BEA will continue.
Figure 5. Helical wheel illustration of residues 11–28 of the mature LL-37. Republished with permission of American Society for Microbiology (Turner et al., 1998); permission conveyed through Copyright Clearance Center, Inc.
Another AMP with promising biofilm eradication activity is oritavancin (Figure 6). Oritavancin is a semi-synthetic lipoglycopeptide, which has been developed for the treatment of medically problematic Gram-positive infections, such as methicillin-susceptible S. aureus (MSSA), methicillin-resistant S. aureus (MRSA), and vancomycin-resistant S. aureus (VRSA) (Allen, 2010). Moeck and coworkers demonstrated that oritavancin possessed both impressive planktonic and biofilm eradication activity (Belley et al., 2009). Oritavancin was able to completely eradicate (99.9%) MSSA, MRSA, and VRSA biofilms at concentrations between 0.3 and 4.5 μM. Most importantly, the concertation required to completely eradicate established biofilms were within one doubling dilution of the respective concertation required to kill planktonic cells of the same strain. Thus, it appears that the activity of oritavancin is not significantly diminished by the formation of a biofilm. Interestingly, oritavancin, which is a structurally related analog of vancomycin, is significantly less toxic to humans than other lipoglycopeptides, such as vancomycin and telavancin (Darpo et al., 2010). This property along with the high potency of this AMP certainly suggests that oritavancin is a promising BEA, at least against Gram-positive pathogens.
While several other AMPs have exhibited some level of biofilm eradication activity (Wei et al., 2006; Beckloff et al., 2007; Hou et al., 2010), most AMPs appear to exhibit more potent anti-biofilm action (inhibition or dispersal) than biofilm eradication activity (Overhage et al., 2008; Flemming et al., 2009; Hou et al., 2009). Consequently, many AMPs are often utilized in combination with antimicrobial treatment (Dashper et al., 2005; Eckert et al., 2006). For example, G10KHc, a novispirin G10 derived AMP, acted synergistically with tobramycin when administered as a co-treatment against P. aeruginosa biofilms (Eckert et al., 2006). Considering the promising anti-biofilm properties of these compounds and their demonstrated synergistic effect with antimicrobials, AMPs represent one promising avenue for the development of treatments for biofilm-related infections. However, as their inherent structures are often quite large and complicated, compared to other antibiotic classes, such as fluoroquinolones and beta-lactams, their modification, development and utilization as BEAs may ultimately be limited.
Quaternary Ammonium Compounds
Quaternary ammonium compounds (QACs) are a large class of broad-spectrum bactericidal agents. Their core structure is amphiphilic comprising a hydrophobic alkyl chain and a hydrophilic quaternary ammonium group, and they are often referred to as AMP mimics, however, their structures are far simpler. Their activity is associated with disruption of the bacterial plasma membrane, which leads to metabolite leakage, and eventual cell lysis (Ioannou et al., 2007). The antibacterial activity of this class of compounds is well-documented, and consequently, many of these types of compounds are already in common commercial use as antiseptics, disinfectants, and preservatives (Russell, 2003). However, their use as BEAs has only recently been explored.
Wuest et al. developed a variety of mono-, bis-, and tris-QACs and demonstrated biofilm eradication activity against pre-formed S. aureus and E. faecalis biofilms (Jennings et al., 2014). In particular, tris-QAC-10 (Figure 7) was able to completely eradicate established biofilms of S. aureus at 50 μM, and E. faecalis at 25 μM (Jennings et al., 2014). While tris-QAC-10 also exhibiting potent planktonic activity against E. coli and P. aeruginosa (MIC 0.5 and 1 μM, respectively), its biofilm eradication activity against these Gram-negative species was not investigated (Jennings et al., 2014). The reported QACs exhibited significant eukaryotic cell toxicity, with authors noting that the development of less toxic analogs was currently underway (Jennings et al., 2014). In a follow-up publication by the same group, a set of multiQACs was reported that not only exhibited impressive biofilm eradication activity (complete eradication of S. aureus biofilms at 25 μM) but were also considerably less toxic compared to earlier QACs (Forman et al., 2016). Considering the development of these compounds as BEAs is relatively recent, their potency and spectrum of activity are highly impressive. Providing that human cell toxicity can be reduced further in subsequent derivatives, these compounds are certainly one of the more promising approaches for the development of BEAs.
Another recent study reported on two unique dicationic porphyrin QACs XF-70 and XF-73 (Figure 8) with demonstrated potent planktonic antibacterial activity (Farrell et al., 2010). Chopra et al. evaluated these two QACs for biofilm eradication activity against S. aureus biofilms (Ooi et al., 2010). Both XF-70 and XF-73 completely eradicated pre-formed S. aureus biofilms at a concentration of only 2.6 μM. In addition, XF-70 and XF-73 were also compared to a diverse panel of commonly administered antimicrobial agents and were found to be >128-fold more potent than all other tested agents under the same assay conditions against the same S. aureus strain. Furthermore, in a subsequent study by Love et al., XF-73 demonstrated a remarkably low propensity for inducing bacterial resistance (Farrell et al., 2011). With the impressive properties of these QACs there is little surprise that at the time of writing Destiny Pharma has already completed and passed phase 1 clinical trials with XF-73 (Yendewa et al., 2019).
The biofilm eradication properties of QACs position them as a promising strategy for the treatment of biofilm-related infections, however, their inherent toxicity is still a hurdle which will need to be overcome or may limit their clinical use to mostly topical treatments. Furthermore, much like AMPs, the BEA activity of QACs appears to be far more conducive to the treatment of Gram-positive pathogens as opposed to Gram-negative ones. However, as their structures are considerably less complicated and smaller than AMPs, the potential to synthetically modify their core structures to enhance Gram-negative activity is certainly a more plausible task.
Antimicrobial lipids, which include fatty acids and monoglycerides, are defined as single-chain lipid amphiphiles (Yoon et al., 2018). The antimicrobial properties of these compounds have been known since the 1800s after Koch et al. first documented the antibacterial effects of soap, and later observed that fatty acids could inhibit the growth of Bacillus anthracis the causative pathogen of anthrax (Thormar, 2010). Since then the antimicrobial properties of fatty acids and monoglycerides have been extensively explored (Kabara and Vrable, 1977; Desbois and Smith, 2010; Desbois, 2012). Antimicrobial lipids are known to act through a variety of mechanisms, such as increased membrane permeability, cell lysis, disruption of electron transport chain, and inhibition of bacterial enzymes (Yoon et al., 2018). While the antimicrobial properties of these compounds have been known for some time their use as anti-biofilm agents or BEAs is far more recent.
Marshall and Oh were among the first to investigate the use of the monoglyceride, glycerol monolaurate (Figure 9) for the treatment of biofilms (Oh and Marshall, 1995). They examined the biofilm eradication potential of glycerol monolaurate and heat on the foodborne pathogen Listeria monocytogenes. Glycerol monolaurate (182 μM) combined with heat (65°C) were found to complete eradicate 7-days-old adherent cells (biofilms) with only 5 min of contact time (Oh and Marshall, 1995). In a subsequent publication by Peterson and Schlievert, glycerol monolaurate alone was found to completely eradicate S. aureus and Haemophilus influenzae biofilms at a concentration of 1,822 μM (Schlievert and Peterson, 2012). Recently, Santos et al. developed a glycerol monolaurate nanocapsule that was reduced P. aeruginosa biofilm biomass by up to 78% when administered at a concentration of 228 μM. These studies clearly evidence that glycerol monolaurate has some level of biofilm eradication potential. However, the active concentration required for biofilm eradication is still quite high compared to other BEAs, particularly for some pathogens. Nevertheless, results using glycerol monolaurate certainly suggest that monoglycerides may someday find use as BEAs.
Figure 9. Chemical structures of glycerol monolaurate, docosahexaenoic acid, and eicosapentaenoic acid.
Shu et al. recently explored the biofilm eradication capabilities of the two fatty acids, docosahexaenoic acid and eicosapentaenoic acid (Figure 9) against Porphyromonas gingivalis and Fusobacterium nucleatum biofilms (Sun et al., 2016). Administration of docosahexaenoic acid or eicosapentaenoic acid (100 μM) to mature P. gingivalis biofilms eradicated a significant proportion of the live cell population (61 and 47%, respectively). The same effect was also evident, albeit to a lower degree, for F. nucleatum biofilms (19 and 32%, respectively) (Sun et al., 2016). In a follow-up publication by the same group, these same two fatty acids were assessed for activity against Streptococcus mutans biofilms (Sun et al., 2017). Both docosahexaenoic acid and eicosapentaenoic acid were found to significantly damaged the outer membrane of biofilm residing cells (58.8 and 62.5%, respectively), and consequently reduced biofilm thickness by 19 and 42%, respectively, in S. mutans (Sun et al., 2017). Importantly, several studies have demonstrated that both docosahexaenoic acid and eicosapentaenoic acid are relatively non-toxic to human cells at concentrations up to 100 μM (docosahexaenoic acid) and 200 μM (eicosapentaenoic acid) (Peng et al., 2012; Yang et al., 2013; Sun et al., 2016).
Considering the low toxicity and promising anti-biofilm and biofilm eradication activity of antimicrobial lipids, there is little question that their use as BEAs merits further investigation. However, as both monoglycerides and fatty acids are present in typical human diets the potential for frequent exposure to these compounds and the subsequent development of resistance is something that must be considered and investigated.
Anticancer Drugs Mitomycin C AND Cisplatin
Mitomycin C (Figure 10) is an FDA approved chemotherapy agent with antitumor activity (Doll et al., 1985). It is currently administered for the treatment of a variety of cancers, including cervical, lung, gastric, breast, bladder, head and neck, and pancreatic (Bradner, 2001). Mitomycin C is an amphipathic compound, which enters the cell membrane through passive diffusion (Byfield and Calabro-Jones, 1981) and subsequently initiates DNA crosslinking between adjacent guanine nucleotides (Tomasz, 1995). While the anti-tumor properties of mitomycin C are well-established, its potential as a BEA is only a fairly recent discovery (Kwan et al., 2015). Kwan et al. initially demonstrate that mitomycin C possessed potent planktonic antimicrobial activity against both actively replicating and quiescent (persister) cells against a range of pathogenic bacterial species including E. coli, S. aureus, and P. aeruginosa (Wood et al., 2013). However, the MICs of mitomycin C against the above species were often higher than that of ciprofloxacin (Wood et al., 2013). Interestingly, when mitomycin C was administered to established biofilms of either E. coli O157:H7 or S. aureus ATCC 25219 almost complete eradication resulted (<1 × 101 CFU remaining after treatment, >7-log reduction) (Wood et al., 2013). Conversely, under the same conditions ciprofloxacin was significantly less active than mitomycin C against biofilms of E. coli O157:H7 (>1 × 107 CFU remaining after treatment) or S. aureus ATCC 25219 (>1 × 106 CFU remaining after treatment) (Wood et al., 2013). The biofilm eradication activity of mitomycin C has been attributed to its ability to target and eradicate both actively replicating and persister cells and while encouraging, the concentrations utilized in these experiments (30–40 μM) was significantly higher than the therapeutic concentrations approved for cancer treatment (1.5–6 μM) (Bradner, 2001; Kwan et al., 2015). Thus, the toxicity of these higher concentrations on human health would need to be considered. In an additional study by Wood et al., mitomycin C was also demonstrated to possess potent eradication activity against established Acinetobacter baumanni biofilms; however, the concentrations required in this case were even higher (~750 μM) (Cruz-Muniz et al., 2017).
A second anticancer drug with demonstrated biofilm eradication activity is cisplatin (Figure 10) (Chowdhury et al., 2016; Yuan et al., 2018). Cisplatin is also an FDA approved treatment for head and neck, bladder, ovarian, and testicular cancers (Eastman, 1987). Like mitomycin C, cisplatin is also a DNA crosslinker; however, crosslinks occur mostly on the same strand rather than opposing strands like mitomycin C (Eastman, 1987). Wood and coworkers were the first to document the potent eradication activity of cisplatin against established P. aeruginosa biofilms (<1 × 101 CFU remaining after treatment, >7-log reduction), however, the dose required for this activity was quite high (833 μM) (Chowdhury et al., 2016). In a subsequent study by Nielsen and colleagues, cisplatin was also shown to have potent P. aeruginosa biofilm eradication activity (>1-log reduction) (Yuan et al., 2018). However, complete eradication of biofilms was not observed at the maximum concentration tested (42 μM).
While the biofilm eradication activity of anticancer drugs, such as mitomycin C and cisplatin, might be encouraging, strong consideration must be given to their clinical toxicity. Mitomycin C is known to cause bone marrow damage, lung fibrosis, renal failure, and haemolytic anemia (Doll et al., 1985). Cisplatin can cause bone marrow suppression, kidney damage, hearing impairment, and heart disease (Oun et al., 2018). Interestingly, mitomycin C has also been investigated as a topical treatment for extensive, recurrent conjunctival-corneal squamous cell carcinoma (Shields et al., 2002). In this study, Shields et al. found that mitomycin C was not only highly effective as a topical treatment, but also safe at concentrations up 2.6 mM (Shields et al., 2002). Thus, while anticancer drugs, such as mitomycin C may be too toxic for the treatment of internal biofilm-related infections, they may find use in the treatment of external biofilm-related infections, such as those seen in chronic wounds, diabetic foot ulcers or in skin burns. Furthermore, as both drugs are already FDA-approved and have been in clinical use, they are certainly worth considering as last-resort treatment options for biofilm infections highly recalcintrant to antibiotic therapy.
Phenazines AND Quinolines
Phenazines are redox-active secondary metabolites, which are produced naturally by many Gram-negative and Gram-positive bacterial species for example, P. aeruginosa (Cezairliyan et al., 2013), Streptomyces spp. (Karnetova et al., 1983), and Pantoea agglomerans (Ali et al., 2016). They consist of a dibenzo annulated pyrazine, and the most well-known example (pyocyanin) originates from P. aeruginosa (Lau et al., 2004). Phenazines and their derivatives exhibit activity against both Gram-negative and Gram-positive species; however, Gram-positive species appear to be more susceptible (Baron and Rowe, 1981). Interest in the potential use of phenazines as BEAs arose from the finding that pyocyanin allowed P. aeruginosa biofilm infections to outcompete S. aureus biofilm infections in the lungs of cystic fibrosis patients (Saiman, 2004; Dietrich et al., 2013).
Huigens et al. were the first to investigate the biofilm eradication activity of phenazine based compounds and demonstrate their impressive biofilm eradication activity against S. aureus biofilms (Garrison et al., 2015b). The most potent of these derivatives was bromophenazine-8 (Figure 11) which completely eradicated biofilms at concentrations between 62.5 and 100 μM. In a subsequent publication by the same group, they prepared an additional library of halogenated phenazines, which this time exhibited biofilm eradication activity against several Gram-positive species (S. aureus, Staphylococcus epidermidis and Enterococcus faecium) (Garrison et al., 2015a). Halogenated phenazine-14 (Figure 11) exhibited the most potent biofilm eradication activity against all three pathogens with complete eradication occurring at concentrations between 0.2 and 12 μM (Garrison et al., 2015a). Furthermore, the authors also demonstrated that halogenated phenazines are non-toxic to mammalian cells indicating that these compounds or their derivatives represent promising therapeutic candidates for the treatment of Gram-positive biofilm-related infections (Garrison et al., 2015a). The biofilm eradication activity of halogenated quinolones is impressive, at least against Gram-positive pathogens. However, considering the origins of the core phenazine structure (Gram-negative bacterial species), it is doubtful that the activity of this class of BEA will ever extent to Gram-negative pathogens, such as P. aeruginosa. Furthermore, bacterially derived phenazines, for example, pyocyanin from P. aeruginosa, are well-established virulence factors and key quorum sensing molecules (Lau et al., 2004; Karatuna and Yagci, 2010). Thus, it would also be important to investigate the response of Gram-negative species to these BEAs to ensure that halogenated phenazines do not trigger biofilm formation or increased virulence in bacterial species known to utilize these molecules for quorum sensing. This would be of particular clinical importance in cases where mixed biofilms are typically observed, such as oral and skin infections (Elias and Banin, 2012).
Quinolines are heterocyclic aromatic compounds which bear some structural resemblance to phenazines. However, unlike phenazines, quinolines are generally associated with antimalarial drugs (Foley and Tilley, 1998). Interestingly, the structural similarities between these two compounds have led to quinolines being investigated as BEAs. Huigens et al. utilized a scaffold hopping strategy (Sun et al., 2012) to develop quinolines based on the halogenated phenazine-14 core structure (Abouelhassan et al., 2014). They produced a variety of halogenated quinolines which exhibited biofilm inhibition activity against S. aureus and S. epidermidis but possessed little biofilm eradication activity. In subsequent studies by the same group, they improved the biofilm eradication activity of halogenated phenazines against S. epidermidis and E. faecium (Basak et al., 2015, 2016). Of those, halogenated quinoline-3 (Figure 12) completely eradicated S. epidermidis biofilms at only 3.0 μM, while halogenated quinoline-4 eradicated (Figure 12) E. faecium biofilm at just 1.0 μM (Basak et al., 2015, 2016). The potential of phenazines as biofilm eradication agents was comprehensively reviewed by the same authors recently (Huigens et al., 2019).
Both halogenated phenazines and quinolines have certainly demonstrated potent biofilm eradication activity. However, their activity appears to be limited to the Gram-positive pathogens S. aureus, S. epidermidis, and E. faecium. Despite the impressive activity and low cytotoxicity of these compounds, no in vivo analyses have been conducted to date. Nevertheless, these compounds are some of the most promising BEAs documented thus far.
Nitric Oxide-Releasing Antibiotics
The use of nitric oxide in biofilm dispersal has been well-documented (Barraud et al., 2006, 2015), however, nitric oxide is a notoriously challenging molecule to handle, and thus its administration and delivery to a target site is often difficult. Furthermore, nitric oxide induces biofilm dispersal at specific concentrations that are sub-lethal to bacteria (below MIC), which means treatment with nitric oxide will require subsequent or combinational treatment with an antimicrobial agent to eradicate dispersed cells. To address the issues surrounding the use of nitric oxide, an innovative approach has been to develop antimicrobials which release nitric oxide or a nitric oxide donor upon interaction with the target site. Kelso and team were able to produce a nitric oxide-releasing prodrug based on the cephalosporin core structure (Barraud et al., 2012). Here they covalently linked the nitric oxide donor diazeniumdiolate (NONOate) to the 3′ position of Cefaloram to produce cephalosporin-3′-diazeniumdiolate (Figure 13), which upon interaction with the bacterial enzyme β-lactamase released the nitric oxide donor that subsequently decomposes to release nitric oxide. When cephalosporin-3′-diazeniumdiolate was administered to established P. aeruginosa biofilms, a significant reduction in biofilm-residing cells (70%) was achieved at a concentration of only 10 μM (Barraud et al., 2012). It is not clear however, if these removed cells were killed or remained viable and thus the potential of cephalosporin-3′-diazeniumdiolate as a BEA remains to be demonstrated. Yet this study clearly demonstrated the use of cephalosporin-3′-diazeniumdiolate as a targeted nitric oxide-releasing agent, and more agents have now been reported by the same group that significantly reduce a biofilm population, however, these compounds remain to be tested for biofilm eradication (Yepuri et al., 2013).
In a similar approach, Schoenfisch et al. functionalised an alkyl chain modified poly(amidoamine) (PAMAM) dendrimer with a nitric oxide donor to produce a nitric oxide-releasing antimicrobial agent (Worley et al., 2015). Their lead compounds exhibited a 6-log reduction against P. aeruginosa biofilms and a 4-log reduction against S. aureus biofilms (Worley et al., 2015). Furthermore, most nitric oxide functionalised conjugates were found to be significantly more potent (2-fold) than their non-nitric oxide containing parent molecules (Worley et al., 2015), a result which suggests that the ability to release nitric oxide greatly improved the biofilm eradication activity of these conjugates. Interestingly, these compounds appear to exhibit a dual action which incorporates the anti-biofilm activity of nitric oxide with the antimicrobial activity of the alkyl chain modified PAMAM dendrimers. As such they represent an interesting new class of BEAs which are potentially dual-acting. Such dual-acting BEAs, combine the activity of two individual compounds to produce a single compound which is more effective than either of its comprising moieties.
Nitroxide Functionalised Antibiotics
The use of nitric oxide in the BEAs discussed above is complicated by its requirement for release upon contact with the target site (nitric oxide donors must decompose to release nitric oxide). Thus, an another approach that does not require release from the antimicrobial agent would be to utilize a nitric oxide alternative Recently Fairfull-Smith et al. have utilized this approach in the development of nitroxide functionalised antibiotics as BEAs (Verderosa et al., 2016, 2017, 2019a). Nitroxides are not bound by the same limitations as nitric oxide (such as low stability, high reactivity, and gaseous at room temperature). Thus, nitroxides, which have documented anti-biofilm properties (de la Fuente-Núñez et al., 2013; Boase et al., 2018; Woehlk et al., 2019), do not require a delivery or release system. Consequently, they can be synthetically incorporated or linked to other agents, such as antibiotics, without negatively impacting their anti-biofilm properties.
Fairfull-Smith et al. were the first to produce and demonstrate the biofilm eradication activity of nitroxide functionalised antibiotics (Verderosa et al., 2016). Here they synthesized two different ciprofloxacin-nitroxide hybrids (Figure 14) that showed biofilm eradication efficacy against P. aeruginosa biofilms (Verderosa et al., 2016). Ciprofloxacin-nitroxide-10 eradicated 95% of biofilm-residing cells at only 40 μM. This represented a major improvement over the parent compound ciprofloxacin, which had little to no effect on biofilm-residing cells in the same assay system (Reffuveille et al., 2014). These studies also evidenced the fundamental role of the free radical nitroxide to the activity of the compound as removal of the free radical character from the hybrid compound significantly reduced its activity as a BEA. In a follow up publication by the same group, a second generation of ciprofloxacin-nitroxide hybrids (Figure 15) were produced and shown to be almost twice as potent as the first-generation hybrids (94% eradication at 20 μM) against P. aeruginosa biofilms and also had no mammalian cell toxicity (Verderosa et al., 2017). Recently, Fairfull-Smith et al. produced the third generation of ciprofloxacin-nitroxide hybrids with an optimized nitroxide to antibiotic ratio (Verderosa et al., 2019a). These new hybrids were shown to have improved potency against uropathogenic E. coli biofilms (99.7% eradication at 12.5 μM) (Verderosa et al., 2019a). The mechanism of action of these promising BEAs was recently investigated through the development of profluorescent fluoroquinolone nitroxides (Verderosa et al., 2019c). This was the first demonstration that nitroxide-functionalised fluoroquinolones can enter and eradicate both Gram-negative (P. aeruginosa and E. coli) and Gram-positive pathogen cells (S. aureus and Enterococcus faecalis) (Verderosa et al., 2019c), demonstrating the broad-spectrum potential of this group of BEAs. In a subsequent publication by Totsika et al., the activity of ciprofloxacin-nitroxides-23, ciprofloxacin-nitroxides-25, and ciprofloxacin-nitroxides-27 (Figure 15) were investigated for efficacy against S. aureus biofilms (Verderosa et al., 2019b). Here they found that ciprofloxacin-nitroxide-27 was able to completely (99.9%) eradicate established S. aureus biofilm at a concentration of only 64 μM (Verderosa et al., 2019b).
Figure 15. Chemical structures of ciprofloxacin-nitroxide-23, ciprofloxacin-nitroxide-25, and ciprofloxacin-nitroxide-27.
Overall, nitroxide functionalised antibiotics are highly potent (low μM range), exhibit a broad spectrum of activity, have no or low mammalian cytotoxicity, and are based on the structure of a well-established class of antibiotics (fluoroquinolones), making them attractive BEA candidates. In the future, it would be important to examine if other classes of antibiotics can be successfully functionalised with nitroxides to expand this promising group of BEAs.
Most bacteria in nature exist in the form of biofilms. For the medical profession, biofilms present a considerable challenge, as not only are they associated with most infections in humans, but they are also extremely difficult to treat due to their inherent tolerance to immune responses and antimicrobials. Despite this, most antibiotics are developed and tested against free-living bacteria. Yet our understanding of biofilm formation by several clinically important bacteria and the mechanisms contributing to bacterial antibiotic tolerance has significantly advanced over the past 20 years. This new knowledge has led to the development of several biofilm remediation strategies and the discovery of many promising agents. While the development of anti-biofilm agents that inhibit or disperse biofilms have received significant attention their inherent lack of antimicrobial activity necessitates their use in conjunction with antibiotics, which distances them from offering a clinically reliable standalone solution. The development of BEAs, even though still at early stages, appears capable to address many of these issues with several promising agents already described. The advantage of BEAs is that they do not require supplementation with other drugs and are designed to specifically target biofilm-residing cells. In addition, many BEAs exhibit both anti-biofilm and biofilm eradication activities, such as AMPs and nitroxide functionalised antibiotics. This feature, coupled with their low human cell toxicity, positions BEAs as a potentially complete strategy for the treatment of both planktonic and biofilm-related infections. The BEAs presented in this review exemplify how increasing understanding of biofilm antibiotic tolerance mechanisms can lead to the design and development of new antibiotics that could offer effective solutions against biofilms. As our understanding of these mechanisms continues to improve, so will our ability to develop compounds which can circumvent them. In the near future, research will hopefully unravel the complete mechanisms of biofilm antimicrobial tolerance, and the questions of how to best design and develop new antibiotics will become apparent.
AV, MT, and KF-S conceived the concept of the review. AV drafted the manuscript, searched for updated bibliography, and prepared the figures. AV, KF-S, and MT revised, corrected, and edited the manuscript.
This work was supported by a Queensland University of Technology (QUT) grant (to MT and KF-S) and in part by a Clive and Vera Ramaciotti Health Investment Grant (2017HIG0119 to MT). KF-S was supported by an Australian Research Council Future Fellowship (FT140100746) and MT by a QUT Vice-Chancellor's Research Fellowship.
Conflict of Interest
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
Abouelhassan, Y., Garrison, A. T., Burch, G. M., Wong, W., Norwood, V. M., and Huigens, R. W. III. (2014). Discovery of quinoline small molecules with potent dispersal activity against methicillin-resistant Staphylococcus aureus and Staphylococcus epidermidis biofilms using a scaffold hopping strategy. Bioorg. Med. Chem. Lett. 24, 5076–5080. doi: 10.1016/j.bmcl.2014.09.009
Ali, H. M., El-Shikh, M. S., Salem, M. Z., and M, M. (2016). Isolation of bioactive phenazine-1-carboxamide from the soil bacterium Pantoea agglomerans and study of its anticancer potency on different cancer cell lines. J. AOAC Int. 99, 1233–1239. doi: 10.5740/jaoacint.16-0090
Anderl, J. N., Franklin, M. J., and Stewart, P. S. (2000). Role of antibiotic penetration limitation in Klebsiella pneumoniae biofilm resistance to ampicillin and ciprofloxacin. Antimicrob. Agents Chemother. 44, 1818–1824. doi: 10.1128/AAC.44.7.1818-1824.2000
Anderl, J. N., Zahller, J., Roe, F., and Stewart, P. S. (2003). Role of nutrient limitation and stationary-phase existence in Klebsiella pneumoniae biofilm resistance to ampicillin and ciprofloxacin. Antimicrob. Agents Chemother. 47, 1251–1256. doi: 10.1128/AAC.47.4.1251-1256.2003
Arciola, C. R., Campoccia, D., Speziale, P., Montanaro, L., and Costerton, J. W. (2012). Biofilm formation in Staphylococcus implant infections. A review of molecular mechanisms and implications for biofilm-resistant materials. Biomaterials 33, 5967–5982. doi: 10.1016/j.biomaterials.2012.05.031
Bagge, N., Hentzer, M., Andersen, J. B., Ciofu, O., Givskov, M., and Hoiby, N. (2004a). Dynamics and spatial distribution of beta-lactamase expression in Pseudomonas aeruginosa biofilms. Antimicrob. Agents Chemother. 48, 1168–1174. doi: 10.1128/AAC.48.4.1168-1174.2004
Bagge, N., Schuster, M., Hentzer, M., Ciofu, O., Givskov, M., Greenberg, E. P., et al. (2004b). Pseudomonas aeruginosa biofilms exposed to imipenem exhibit changes in global gene expression and beta-lactamase and alginate production. Antimicrob. Agents Chemother. 48, 1175–1187. doi: 10.1128/AAC.48.4.1175-1187.2004
Barraud, N., Hassett, D. J., Hwang, S.-H., Rice, S. A., Kjelleberg, S., and Webb, J. S. (2006). Involvement of nitric oxide in biofilm dispersal of Pseudomonas aeruginosa. J. Bacteriol. 188, 7344–7353. doi: 10.1128/JB.00779-06
Barraud, N., Kardak, B. G., Yepuri, N. R., Howlin, R. P., Webb, J. S., Faust, S. N., et al. (2012). Cephalosporin-3′-diazeniumdiolates: targeted NO-donor prodrugs for dispersing bacterial biofilms. Angew. Chem. Int. Ed. Engl. 51, 9057–9060. doi: 10.1002/anie.201202414
Barraud, N., Kelso, M. J., Rice, S. A., and Kjelleberg, S. (2015). Nitric oxide: a key mediator of biofilm dispersal with applications in infectious diseases. Curr. Pharm. Des. 21, 31–42. doi: 10.2174/1381612820666140905112822
Barraud, N., Storey, M. V., Moore, Z. P., Webb, J. S., Rice, S. A., and Kjelleberg, S. (2009). Nitric oxide-mediated dispersal in single- and multi-species biofilms of clinically and industrially relevant microorganisms. Microb. Biotechnol. 2, 370–378. doi: 10.1111/j.1751-7915.2009.00098.x
Basak, A., Abouelhassan, Y., and Huigens, R. W. III. (2015). Halogenated quinolines discovered through reductive amination with potent eradication activities against MRSA, MRSE and VRE biofilms. Org. Biomol. Chem. 13, 10290–10294. doi: 10.1039/C5OB01883H
Basak, A., Abouelhassan, Y., Norwood IV, V. M., Bai, F., Nguyen, M. T., Jin, S., et al. (2016). Synthetically tuning the 2-position of halogenated quinolines: optimizing antibacterial and biofilm eradication activities via alkylation and reductive amination pathways. Chem. Eur. J. 22, 9181–9189. doi: 10.1002/chem.201600926
Bazaka, K., Jacob, M. V., Crawford, R. J., and Ivanova, E. P. (2012). Efficient surface modification of biomaterial to prevent biofilm formation and the attachment of microorganisms. Appl. Microbiol. Biotechnol. 95, 299–311. doi: 10.1007/s00253-012-4144-7
Beckloff, N., Laube, D., Castro, T., Furgang, D., Park, S., Perlin, D., et al. (2007). Activity of an antimicrobial peptide mimetic against planktonic and biofilm cultures of oral pathogens. Antimicrob. Agents Chemother. 51:4125. doi: 10.1128/AAC.00208-07
Belley, A., Neesham-Grenon, E., McKay, G., Arhin, F. F., Harris, R., Beveridge, T., et al. (2009). Oritavancin kills stationary-phase and biofilm Staphylococcus aureus cells in vitro. Antimicrob. Agents Chemother. 53:918. doi: 10.1128/AAC.00766-08
Boase, N. R. B., Torres, M. D. T., Fletcher, N. L., de la Fuente-Nunez, C., and Fairfull-Smith, K. E. (2018). Polynitroxide copolymers to reduce biofilm fouling on surfaces. Polym. Chem. 9, 5308–5318. doi: 10.1039/C8PY01101J
Borriello, G., Werner, E., Roe, F., Kim, A. M., Ehrlich, G. D., and Stewart, P. S. (2004). Oxygen limitation contributes to antibiotic tolerance of Pseudomonas aeruginosa in biofilms. Antimicrob. Agents Chemother. 48, 2659–2664. doi: 10.1128/AAC.48.7.2659-2664.2004
Campanac, C., Pineau, L., Payard, A., Baziard-Mouysset, G., and Roques, C. (2002). Interactions between biocide cationic agents and bacterial biofilms. Antimicrob. Agents Chemother. 46, 1469–1474. doi: 10.1128/AAC.46.5.1469-1474.2002
Campoccia, D., Montanaro, L., and Arciola, C. R. (2013). A review of the biomaterials technologies for infection-resistant surfaces. Biomaterials 34, 8533–8554. doi: 10.1016/j.biomaterials.2013.07.089
Cezairliyan, B., Vinayavekhin, N., Grenfell-Lee, D., Yuen, G. J., Saghatelian, A., and Ausubel, F. M. (2013). Identification of Pseudomonas aeruginosa phenazines that kill Caenorhabditis elegans. PLoS Pathog. 9:e1003101. doi: 10.1371/journal.ppat.1003101
Chennupati, S. K., Chiu, A. G., Tamashiro, E., Banks, C. A., Cohen, M. B., Bleier, B. S., et al. (2009). Effects of an LL-37-derived antimicrobial peptide in an animal model of biofilm Pseudomonas sinusitis. Am. J. Rhinol. Allergy 23, 46–51. doi: 10.2500/ajra.2009.23.3261
Chowdhury, N., Wood, T. L., Martinez-Vazquez, M., Garcia-Contreras, R., and Wood, T. K. (2016). DNA-crosslinker cisplatin eradicates bacterial persister cells. Biotechnol. Bioeng. 113, 1984–1992. doi: 10.1002/bit.25963
Costerton, J. W., Cheng, K. J., Geesey, G. G., Ladd, T. I., Nickel, J. C., Dasgupta, M., et al. (1987). Bacterial biofilms in nature and disease. Annu. Rev. Microbiol. 41, 435–464. doi: 10.1146/annurev.mi.41.100187.002251
Cruz-Muniz, M. Y., Lopez-Jacome, L. E., Hernandez-Duran, M., Franco-Cendejas, R., Licona-Limon, P., Ramos-Balderas, J. L., et al. (2017). Repurposing the anticancer drug mitomycin C for the treatment of persistent Acinetobacter baumannii infections. Int. J. Antimicrob. Agents 49, 88–92. doi: 10.1016/j.ijantimicag.2016.08.022
Darpo, B., Lee, S. K., Moon, T. E., Sills, N., and Mason, J. W. (2010). Oritavancin, a new lipoglycopeptide antibiotic: results from a thorough QT study. J. Clin. Pharmacol. 50, 895–903. doi: 10.1177/0091270009355449
Dashper, S. G., Brien-Simpson, N. M., Cross, K. J., Paolini, R. A., Hoffmann, B., Catmull, D. V., et al. (2005). Divalent metal cations increase the activity of the antimicrobial peptide kappacin. Antimicrob. Agents Chemother. 49:2322. doi: 10.1128/AAC.49.6.2322-2328.2005
Davenport, E. K., Call, D. R., and Beyenal, H. (2014). Differential protection from tobramycin by extracellular polymeric substances from Acinetobacter baumannii and Staphylococcus aureus biofilms. Antimicrob. Agents Chemother. 58, 4755–4761. doi: 10.1128/AAC.03071-14
de la Fuente-Núñez, C., Reffuveille, F., Fairfull-Smith, K. E., and Hancock, R. E. W. (2013). Effect of nitroxides on swarming motility and biofilm formation, multicellular behaviors in Pseudomonas aeruginosa. Antimicrob. Agents Chemother. 57, 4877–4881. doi: 10.1128/AAC.01381-13
Delcaru, C., Alexandru, I., Podgoreanu, P., Grosu, M., Stavropoulos, E., Chifiriuc, M. C., et al. (2016). Microbial biofilms in urinary tract infections and prostatitis: etiology, pathogenicity, and combating strategies. Pathogens 5:65. doi: 10.3390/pathogens5040065
Desbois, A. P. (2012). Potential applications of antimicrobial fatty acids in medicine, agriculture and other industries. Recent Pat. Antiinfect. Drug Discov. 7, 111–122. doi: 10.2174/157489112801619728
Desbois, A. P., and Smith, V. J. (2010). Antibacterial free fatty acids: activities, mechanisms of action and biotechnological potential. Appl. Microbiol. Biotechnol. 85, 1629–1642. doi: 10.1007/s00253-009-2355-3
Dietrich, L. E. P., Okegbe, C., Price-Whelan, A., Sakhtah, H., Hunter, R. C., and Newman, D. K. (2013). Bacterial community morphogenesis is intimately linked to the intracellular redox state. J. Bacteriol. 195:1371. doi: 10.1128/JB.02273-12
Eckert, R., Brady, K. M., Greenberg, E. P., Qi, F., Yarbrough, D. K., He, J., et al. (2006). Enhancement of antimicrobial activity against Pseudomonas aeruginosa by coadministration of G10KHc and tobramycin. Antimicrob. Agents Chemother. 50:3833. doi: 10.1128/AAC.00509-06
Farrell, D. J., Robbins, M., Rhys-Williams, W., and Love, W. G. (2010). In vitro activity of XF-73, a novel antibacterial agent, against antibiotic-sensitive and -resistant Gram-positive and Gram-negative bacterial species. Int. J. Antimicrob. Agents 35, 531–536. doi: 10.1016/j.ijantimicag.2010.02.008
Farrell, D. J., Robbins, M., Rhys-Williams, W., and Love, W. G. (2011). Investigation of the potential for mutational resistance to XF-73, retapamulin, mupirocin, fusidic acid, daptomycin, and vancomycin in methicillin-resistant Staphylococcus aureus isolates during a 55-passage study. Antimicrob. Agents Chemother. 55:1177. doi: 10.1128/AAC.01285-10
Field, T. R., White, A., Elborn, J. S., and Tunney, M. M. (2005). Effect of oxygen limitation on the in vitro antimicrobial susceptibility of clinical isolates of Pseudomonas aeruginosa grown planktonically and as biofilms. Eur. J. Clin. Microbiol. Infect. Dis. 24, 677–687. doi: 10.1007/s10096-005-0031-9
Flemming, K., Klingenberg, C., Cavanagh, J. P., Sletteng, M., Stensen, W., Svendsen, J. S., et al. (2009). High in vitro antimicrobial activity of synthetic antimicrobial peptidomimetics against staphylococcal biofilms. J. Antimicrob. Chemother. 63, 136–145. doi: 10.1093/jac/dkn464
Forman, M. E., Jennings, M. C., Wuest, W. M., and Minbiole, K. P. (2016). Building a better quaternary ammonium compound (QAC): branched tetracationic antiseptic amphiphiles. Chem. Med. Chem. 11, 1401–1405. doi: 10.1002/cmdc.201600176
Garrison, A. T., Abouelhassan, Y., Kallifidas, D., Bai, F., Ukhanova, M., Mai, V., et al. (2015a). Halogenated phenazines that potently eradicate biofilms, MRSA persister cells in non-biofilm cultures, and Mycobacterium tuberculosis. Angew. Chem. Int. Ed. Engl. 54, 14819–14823. doi: 10.1002/anie.201508155
Garrison, A. T., Bai, F., Abouelhassan, Y., Paciaroni, N. G., Jin, S., and Huigens III, R. W. (2015b). Bromophenazine derivatives with potent inhibition, dispersion and eradication activities against Staphylococcus aureus biofilms. RSC Adv. 5, 1120–1124. doi: 10.1039/C4RA08728C
Gordon, Y. J., Huang, L. C., Romanowski, E. G., Yates, K. A., Proske, R. J., and McDermott, A. M. (2005). Human cathelicidin (LL-37), a multifunctional peptide, is expressed by ocular surface epithelia and has potent antibacterial and antiviral activity. Curr. Eye Res. 30, 385–394. doi: 10.1080/02713680590934111
Guilhen, C., Forestier, C., and Balestrino, D. (2017). Biofilm dispersal: multiple elaborate strategies for dissemination of bacteria with unique properties. Mol. Microbiol. 105, 188–210. doi: 10.1111/mmi.13698
Hannan, S., Ready, D., Jasni, A. S., Rogers, M., Pratten, J., and Roberts, A. P. (2010). Transfer of antibiotic resistance by transformation with eDNA within oral biofilms. FEMS Immunol. Med. Microbiol. 59, 345–349. doi: 10.1111/j.1574-695X.2010.00661.x
Harrison, J. J., Ceri, H., Roper, N. J., Badry, E. A., Sproule, K. M., and Turner, R. J. (2005a). Persister cells mediate tolerance to metal oxyanions in Escherichia coli. Microbiology 151, 3181–3195. doi: 10.1099/mic.0.27794-0
Harrison, J. J., Turner, R. J., and Ceri, H. (2005b). Persister cells, the biofilm matrix and tolerance to metal cations in biofilm and planktonic Pseudomonas aeruginosa. Environ. Microbiol. 7, 981–994. doi: 10.1111/j.1462-2920.2005.00777.x
Hell, E., Giske, C. G., Nelson, A., Romling, U., and Marchini, G. (2010). Human cathelicidin peptide LL37 inhibits both attachment capability and biofilm formation of Staphylococcus epidermidis. Lett. Appl. Microbiol. 50, 211–215. doi: 10.1111/j.1472-765X.2009.02778.x
Hou, S., Liu, Z., Young, A. W., Mark, S. L., Kallenbach, N. R., and Ren, D. (2010). Effects of Trp- and Arg-containing antimicrobial-peptide structure on inhibition of Escherichia coli planktonic growth and biofilm formation. Appl. Environ. Microbiol. 76, 1967–1974. doi: 10.1128/AEM.02321-09
Hou, S., Zhou, C., Liu, Z., Young, A. W., Shi, Z., Ren, D., et al. (2009). Antimicrobial dendrimer active against Escherichia coli biofilms. Bioorg. Med. Chem. Lett. 19, 5478–5481. doi: 10.1016/j.bmcl.2009.07.077
Ioannou, C. J., Hanlon, G. W., and Denyer, S. P. (2007). Action of disinfectant quaternary ammonium compounds against Staphylococcus aureus. Antimicrob. Agents Chemother. 51, 296–306. doi: 10.1128/AAC.00375-06
Jennings, M. C., Ator, L. E., Paniak, T. J., Minbiole, K. P., and Wuest, W. M. (2014). Biofilm-eradicating properties of quaternary ammonium amphiphiles: simple mimics of antimicrobial peptides. Chem. Bio. Chem. 15, 2211–2215. doi: 10.1002/cbic.201402254
Karatuna, O., and Yagci, A. (2010). Analysis of quorum sensing-dependent virulence factor production and its relationship with antimicrobial susceptibility in Pseudomonas aeruginosa respiratory isolates. Clin. Microbiol. Infect. 16, 1770–1775. doi: 10.1111/j.1469-0691.2010.03177.x
Katsikogianni, M., and Missirlis, Y. F. (2004). Concise review of mechanisms of bacterial adhesion to biomaterials and of techniques used in estimating bacteria-material interactions. Eur. Cell Mater. 8, 37–57. doi: 10.22203/eCM.v008a05
Keren, I., Shah, D., Spoering, A., Kaldalu, N., and Lewis, K. (2004b). Specialized persister cells and the mechanism of multidrug tolerance in Escherichia coli. J. Bacteriol. 186, 8172–8180. doi: 10.1128/JB.186.24.8172-8180.2004
Lebeaux, D., Ghigo, J.-M., and Beloin, C. (2014). Biofilm-related infections: bridging the gap between clinical management and fundamental aspects of recalcitrance toward antibiotics. Microbiol. Mol. Biol. Rev. 78, 510–543. doi: 10.1128/MMBR.00013-14
Luppens, S. B. I., Reij, M. W., van der Heijden, R. W. L., Rombouts, F. M., and Abee, T. (2002). Development of a standard test to assess the resistance of Staphylococcus aureus biofilm cells to disinfectants. Appl. Environ. Microbiol. 68, 4194–4200. doi: 10.1128/AEM.68.9.4194-4200.2002
Machado, D., Castro, J., Palmeira-de-Oliveira, A., Martinez-de-Oliveira, J., and Cerca, N. (2016). Bacterial vaginosis biofilms: challenges to current therapies and emerging solutions. Front. Microbiol. 6:1528. doi: 10.3389/fmicb.2015.01528
Marvasi, M., Chen, C., Carrazana, M., Durie, I. A., and Teplitski, M. (2014). Systematic analysis of the ability of nitric oxide donors to dislodge biofilms formed by Salmonella enterica and Escherichia coli O157:H7. AMB Express 4, 1–11. doi: 10.1186/s13568-014-0042-y
McDougald, D., Rice, S. A., Barraud, N., Steinberg, P. D., and Kjelleberg, S. (2012). Should we stay or should we go: mechanisms and ecological consequences for biofilm dispersal. Nat. Rev. Microbiol. 10, 39–50. doi: 10.1038/nrmicro2695
Nablo, B. J., Rothrock, A. R., and Schoenfisch, M. H. (2005). Nitric oxide-releasing sol–gels as antibacterial coatings for orthopedic implants. Biomaterials 26, 917–924. doi: 10.1016/j.biomaterials.2004.03.031
Ooi, N., Miller, K., Randall, C., Rhys-Williams, W., Love, W., and Chopra, I. (2010). XF-70 and XF-73, novel antibacterial agents active against slow-growing and non-dividing cultures of Staphylococcus aureus including biofilms. J. Antimicrob. Chemother. 65, 72–78. doi: 10.1093/jac/dkp409
Overhage, J., Campisano, A., Bains, M., Torfs, E. C., Rehm, B. H., and Hancock, R. E. (2008). Human host defense peptide LL-37 prevents bacterial biofilm formation. Infect. Immun. 76, 4176–4182. doi: 10.1128/IAI.00318-08
Penesyan, A., Gillings, M., and Paulsen, I. T. (2015). Antibiotic discovery: combatting bacterial resistance in cells and in biofilm communities. Molecules 20, 5286–5298. doi: 10.3390/molecules20045286
Peng, Y., Zheng, Y., Zhang, Y., Zhao, J., Chang, F., Lu, T., et al. (2012). Different effects of omega-3 fatty acids on the cell cycle in C2C12 myoblast proliferation. Mol. Cell. Biochem. 367, 165–173. doi: 10.1007/s11010-012-1329-4
Rachid, S., Ohlsen, K., Witte, W., Hacker, J., and Ziebuhr, W. (2000). Effect of subinhibitory antibiotic concentrations on polysaccharide intercellular adhesin expression in biofilm-forming Staphylococcus epidermidis. Antimicrob. Agents Chemother. 44, 3357–3363. doi: 10.1128/AAC.44.12.3357-3363.2000
Redelman, C. V., Chakravarty, S., and Anderson, G. G. (2014). Antibiotic treatment of Pseudomonas aeruginosa biofilms stimulates expression of the magnesium transporter gene mgtE. Microbiology 160, 165–178. doi: 10.1099/mic.0.070144-0
Reffuveille, F., de la Fuente-Núñez, C., Hancock, R. E. W., and Fairfull-Smith, K. E. (2015). Potentiation of ciprofloxacin action against gram-negative bacterial biofilms by a nitroxide. Pathog. Dis. 73:ftv016. doi: 10.1093/femspd/ftv016
Reffuveille, F., de la Fuente-Nunez, C., Mansour, S., and Hancock, R. E. (2014). A broad-spectrum antibiofilm peptide enhances antibiotic action against bacterial biofilms. Antimicrob. Agents Chemother. 58, 5363–5371. doi: 10.1128/AAC.03163-14
Roizman, D., Vidaillac, C., Givskov, M., and Yang, L. (2017). In vitro evaluation of biofilm dispersal as a therapeutic strategy to restore antimicrobial efficacy. Antimicrob. Agents Chemother. 61, e01088–e01017. doi: 10.1128/AAC.01088-17
Roy, R., Tiwari, M., Donelli, G., and Tiwari, V. (2018). Strategies for combating bacterial biofilms: a focus on anti-biofilm agents and their mechanisms of action. Virulence 9, 522–554. doi: 10.1080/21505594.2017.1313372
Russell, A. D. (2003). Biocide use and antibiotic resistance: the relevance of laboratory findings to clinical and environmental situations. Lancet Infect. Dis. 3, 794–803. doi: 10.1016/S1473-3099(03)00833-8
Sailer, F. C., Meberg, B. M., and Young, K. D. (2003). beta-Lactam induction of colanic acid gene expression in Escherichia coli. FEMS Microbiol. Lett. 226, 245–249. doi: 10.1016/S0378-1097(03)00616-5
Shai, Y. (1999). Mechanism of the binding, insertion and destabilization of phospholipid bilayer membranes by alpha-helical antimicrobial and cell non-selective membrane-lytic peptides. Biochim. Biophys. Acta 1462, 55–70. doi: 10.1016/S0005-2736(99)00200-X
Shields, C. L., Naseripour, M., and Shields, J. A. (2002). Topical mitomycin C for extensive, recurrent conjunctival-corneal squamous cell carcinoma. Am. J. Ophthalmol. 133, 601–606. doi: 10.1016/S0002-9394(02)01400-9
Spoering, A. L., and Lewis, K. (2001). Biofilms and planktonic cells of Pseudomonas aeruginosa have similar resistance to killing by antimicrobials. J. Bacteriol. 183, 6746–6751. doi: 10.1128/JB.183.23.6746-6751.2001
Stone, G., Wood, P., Dixon, L., Keyhan, M., and Matin, A. (2002). Tetracycline rapidly reaches all the constituent cells of uropathogenic Escherichia coli biofilms. Antimicrob. Agents Chemother. 46, 2458–2461. doi: 10.1128/AAC.46.8.2458-2461.2002
Sun, M., Dong, J., Xia, Y., and Shu, R. (2017). Antibacterial activities of docosahexaenoic acid (DHA) and eicosapentaenoic acid (EPA) against planktonic and biofilm growing Streptococcus mutans. Microb. Pathog. 107, 212–218. doi: 10.1016/j.micpath.2017.03.040
Sun, M., Zhou, Z., Dong, J., Zhang, J., Xia, Y., and Shu, R. (2016). Antibacterial and antibiofilm activities of docosahexaenoic acid (DHA) and eicosapentaenoic acid (EPA) against periodontopathic bacteria. Microb. Pathog. 99, 196–203. doi: 10.1016/j.micpath.2016.08.025
Thormar, H. (2010). “Antibacterial effects of lipids: historical review (1881 to 1960),” in Lipids and Essential Oils as Antimicrobial Agents, ed H. Thormar, (Hoboken, NJ: Wiley), 25–45. doi: 10.1002/9780470976623.ch2
Turner, J., Cho, Y., Dinh, N.-N., Waring, A. J., and Lehrer, R. I. (1998). Activities of LL-37, a cathelin-associated antimicrobial peptide of human neutrophils. Antimicrob. Agents Chemother. 42:2206. doi: 10.1128/AAC.42.9.2206
Verderosa, A., Harris, J., Dhouib, R., Totsika, M., and Fairfull-Smith, K. (2019a). Eradicating uropathogenic Escherichia coli biofilms with a ciprofloxacin-dinitroxide conjugate. Med. Chem. Comm. 10, 699–711. doi: 10.1039/C9MD00062C
Verderosa, A. D., de la Fuente-Núñez, C., Mansour, S. C., Cao, J., Lu, T. K., Hancock, R. E. W., et al. (2017). Ciprofloxacin-nitroxide hybrids with potential for biofilm control. Eur. J. Med. Chem. 138, 590–601. doi: 10.1016/j.ejmech.2017.06.058
Verderosa, A. D., Dhouib, R., Fairfull-Smith, K. E., and Totsika, M. (2019b). Nitroxide functionalized antibiotics are promising eradication agents against Staphylococcus aureus biofilms. Antimicrob. Agents Chemother. doi: 10.1128/AAC.01685-19. [Epub ahead of print].
Verderosa, A. D., Dhouib, R., Fairfull-Smith, K. E., and Totsika, M. (2019c). Profluorescent fluoroquinolone-nitroxides for investigating antibiotic–bacterial interactions. Antibiotics 8:E19. doi: 10.3390/antibiotics8010019
Verderosa, A. D., Mansour, S. C., de la Fuente-Núñez, C., Hancock, R. E., and Fairfull-Smith, K. E. (2016). Synthesis and evaluation of ciprofloxacin-nitroxide conjugates as anti-biofilm agents. Molecules 21:841. doi: 10.3390/molecules21070841
Vieira Colombo, A. P., Magalhães, C. B., Hartenbach, F. A., Martins do Souto, R., and Maciel da Silva-Boghossian, C. (2016). Periodontal-disease-associated biofilm: a reservoir for pathogens of medical importance. Microbial. Pathog. 94, 27–34. doi: 10.1016/j.micpath.2015.09.009
von Rosenvinge, E. C., O'May, G. A., Macfarlane, S., Macfarlane, G. T., and Shirtliff, M. E. (2013). Microbial biofilms and gastrointestinal diseases. Pathog. Dis. 67, 25–38. doi: 10.1111/2049-632X.12020
Walters, M. C. III., Roe, F., Bugnicourt, A., Franklin, M. J., and Stewart, P. (2003). Contributions of antibiotic penetration, oxygen limitation, and low metabolic activity to tolerance of Pseudomonas aeruginosa biofilms to ciprofloxacin and tobramycin. Antimicrob. Agents Chemother. 47, 317–323. doi: 10.1128/AAC.47.1.317-323.2003
Wei, G. X., Campagna, A. N., and Bobek, L. A. (2006). Effect of MUC7 peptides on the growth of bacteria and on Streptococcus mutans biofilm. J. Antimicrob. Chemother. 57, 1100–1109. doi: 10.1093/jac/dkl120
Woehlk, H., Trimble, M. J., Mansour, S. C., Pletzer, D., Trouillet, V., Welle, A., et al. (2019). Controlling biofilm formation with nitroxide functional surfaces. Polym. Chem. 10, 4252–4258. doi: 10.1039/C9PY00690G
Worley, B. V., Schilly, K. M., and Schoenfisch, M. H. (2015). Anti-biofilm efficacy of dual-action nitric oxide-releasing alkyl chain modified poly(amidoamine) dendrimers. Mol. Pharm. 12, 1573–1583. doi: 10.1021/acs.molpharmaceut.5b00006
Yang, Y. C., Lii, C. K., Wei, Y. L., Li, C. C., Lu, C. Y., Liu, K. L., et al. (2013). Docosahexaenoic acid inhibition of inflammation is partially via cross-talk between Nrf2/heme oxygenase 1 and IKK/NF-kappaB pathways. J. Nutr. Biochem. 24, 204–212. doi: 10.1016/j.jnutbio.2012.05.003
Yendewa, G. A., Griffiss, J. M., Jacobs, M. R., Fulton, S. A., O'Riordan, M. A., Gray, W. A., et al. (2019). A two-part phase I study to establish and compare the safety and local tolerability of two nasal formulations of XF-73 for decolonization of Staphylococcus aureus: a previously investigated 0.5 mg/g viscosified gel formulation versus a modified formulation. J. Glob. Antimicrob. Resist. doi: 10.1016/j.jgar.2019.09.017. [Epub ahead or print].
Yepuri, N. R., Barraud, N., Mohammadi, N. S., Kardak, B. G., Kjelleberg, S., Rice, S. A., et al. (2013). Synthesis of cephalosporin-3′-diazeniumdiolates: biofilm dispersing NO-donor prodrugs activated by beta-lactamase. Chem. Commun. (Camb). 49, 4791–4793. doi: 10.1039/c3cc40869h
Yoon, B. K., Jackman, J. A., Valle-González, E. R., and Cho, N.-J. (2018). Antibacterial free fatty acids and monoglycerides: biological activities, experimental testing, and therapeutic applications. Int. J. Mol. Sci. 19:1114. doi: 10.3390/ijms19041114
Yuan, M., Chua, S. L., Liu, Y., Drautz-Moses, D. I., Yam, J. K. H., Aung, T. T., et al. (2018). Repurposing the anticancer drug cisplatin with the aim of developing novel Pseudomonas aeruginosa infection control agents. Beilstein J. Org. Chem. 14, 3059–3069. doi: 10.3762/bjoc.14.284
Keywords: antibiotics, bacteria, biofilm, biofilm antibiotic tolerance, biofilm eradication agent, infection, resistance
Citation: Verderosa AD, Totsika M and Fairfull-Smith KE (2019) Bacterial Biofilm Eradication Agents: A Current Review. Front. Chem. 7:824. doi: 10.3389/fchem.2019.00824
Received: 02 September 2019; Accepted: 12 November 2019;
Published: 28 November 2019.
Edited by:Nenad Filipović, Faculty of Agriculture, University of Belgrade, Serbia
Reviewed by:Fany Reffuveille, Université de Reims Champagne-Ardenne, France
Jelena Lozo, Faculty of Biology, University of Belgrade, Serbia
Copyright © 2019 Verderosa, Totsika and Fairfull-Smith. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Anthony D. Verderosa, firstname.lastname@example.org