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Logo of nihpaAbout Author manuscriptsSubmit a manuscriptHHS Public Access; Author Manuscript; Accepted for publication in peer reviewed journal;
 
Future Microbiol. Author manuscript; available in PMC 2010 April 1.
Published in final edited form as:
PMCID: PMC2827931
NIHMSID: NIHMS171783

Clinical and laboratory evidence for Neisseria meningitidis biofilms

Abstract

Neisseria meningitidis is the etiologic agent of meningococcal meningitis. Carriage of the organism is approximately 10% while active disease occurs at a rate of 1:100,000. Recent publications demonstrate that N. meningitidis has the ability to form biofilms on glass, plastic or cultured human bronchial epithelial cells. Microcolony-like structures are also observed in histological sections from patients with active meningococcal disease. This review investigates the possible role of meningococcal biofilms in carriage and active disease, based on the laboratory and clinical aspects of the disease.

Keywords: biofilm, capsule, HrpA, Neisseria meningitidis, two-partner secretion

Bacterial biofilms

Biofilm research has gained considerable attention in the last 10–15 years in both the clinical and research communities. A biofilm is a community of microorganisms attached to a surface and encased in an exopolymeric matrix. Biofilms are formed under conditions of environmental stress, and are often associated with shear forces. The members of the biofilm are afforded more protection from environmental factors than if they were in an individual planktonic state. This includes protection from antimicrobials, changes in osmolarity, predation, UV light, reactive oxygen species and dehydration [1]. This added protection allows the bacteria living in the biofilm to persist in environs such as water pipes in industrial settings, as well as in the human host in chronic infections. A model organism for biofilm development is Pseudomonas aeruginosa, which forms biofilms in the lungs of cystic fibrosis patients. For this organism, biofilm formation occurs in five stages:

  • Loose association of the bacterium with a surface;
  • Tight bacterial adherence and transcriptional changes to adapt to the new environment;
  • Bacterial aggregation and microcolony formation, as defined by a small number of bacteria encased in a matrix;
  • Mature biofilm development, often seen as mats or tall structures that have channels to disperse nutrients to all the bacteria;
  • Detachment of bacteria from the biofilm to colonize other locations [1].

The importance of biofilms in infectious disease was established when it was demonstrated that the biofilm phenotype endows an increased level of antibiotic resistance [2]. There are various hypotheses as to why biofilms promote antibiotic resistance. The first is that the matrix traps antibiotics or possibly other host immunodefensive substances, such as immunoglobulins, complement components and reactive oxygen or nitrogen species [2]. This would protect bacteria on the inside of the biofilm but still may sacrifice bacteria on the outer portions of the biofilm. The second way biofilms could aid in antibiotic resistance is that some members of the biofilm take on characteristics of stationary-phase bacteria where metabolism is reduced to low levels [2]. Many antibiotics act on metabolic pathways and would therefore have little affect on a quiescent bacterium within a biofilm. The third mechanism through which biofilms resist antibiotics is with persisters [2]. These are bacteria that have natural resistance to the antibiotic or other adverse environmental conditions and would therefore survive even if the other members of the biofilm perish. The final mechanism is related to the third. Biofilms of P. aeruginosa contain DNA in their matrix and genetic transfer between organisms in the biofilm is established [3,4]. The biofilm sets up an environment where DNA from the matrix or conjugation with adjacent bacteria could provide a source of antibiotic resistance genes and therefore increase the chances of survival to members of the biofilm population.

Biofilms are implicated in several infectious diseases and merit study to reduce morbidity. The biofilm state is often associated with chronic infections and not acute infections. In cystic fibrosis, chronic lung infections are due to P. aeruginosa, Staphylococcus aureus and Haemophilus influenzae, which reside in the airway in biofilms [5,6]. Otitis media is caused by nontypeable H. influenzae living within a biofilm [7]. Endocarditis is considered to be a biofilm-related infection caused by staphylococci or streptococci, and urinary tract infections are often caused by biofilms formed by uropathogenic Escherichia coli, Proteus mirabilis or Klebsiella pneumoniae [8,9]. Implant- and catheter-related infections are caused by many of the aforementioned organisms [8].

Biofilm formation by pathogenic Neisseria

Neisseria spp. are obligate human pathogens/commensals. The nasopharyngeal flora members, Neisseria meningitidis and Neisseria lactamica, are able to infect the human hosts for long periods of time without obvious symptomatic disease [10,11]. Likewise, infection by Neisseria gonorrhoeae often results in long-term asymptomatic infections in women [12]. The ability to survive for long periods of time in the human host despite a response by both innate- and adaptive-immune defense mechanisms, indicates a specialized lifestyle that resists clearance. The authors hypothesize that Neisseria spp. carriage in the human host is made possible by its ability to form biofilms on human mucosa. A brief overview of the literature pertaining to what is known regarding biofilms formed by N. gonorrhoeae is given below. A detailed review of the literature pertaining to N. meningitidis biofilms and clinical data that may indicate the relevance of N. meningitidis biofilms in the infection and carriage process will be discussed later in the text.

N. gonorrhoeae biofilms

N. gonorrhoeae (gonococcus) is the etiologic cause of the sexually transmitted disease, gonorrhea. In men, gonococcal infection results in acute urethritis 2–5 days postinfection [12]. In women, gonococcal infection is often asymptomatic. The undetected infection can ascend the female genital tract and cause more serious infections such as pelvic inflammatory disease, which can lead to sterility. The ascending infection can also escape the female reproductive tract to cause disseminated gonococcal infection [12].

The ability of the gonococcus to remain undetected in women led to speculation that N. gonorrhoeae persists as a biofilm. Gonococcal biofilms can form in vitro on cervical tissue and can persist up to 8 days without obvious damage to the cervical tissue [13]. These biofilms are also maintained in a flow cell on glass [13]. Gonococcal biofilms are observed in vivo on cervical biopsies, as well as in mixed biofilms on indwelling intrauterine devices of women with reproductive tract infections [14,15].

Electron micrographs of gonococcal or meningococcal biofilms show the presence of long membrane-like structures throughout biofilms grown in vitro on glass or on transformed human airway epithelia in flow cells, as well as on archival cervical biopsies of gonococcal culture-positive patients (Figure 1). These membrane-like structures on the gonococcal biofilms label with antibody 2C3, which reacts to the outer membrane protein H.8 present in both the gonococcus and meningococcus [15]. The pathogenic Neisseria are known to bleb the outer membrane and release it into the extracellular environment. A mutation in the msbB gene results in a penta-acyl lipid A and has a reduced ability to blebbing. This mutant also has a reduced ability to form biofilms in flow cells [15]. The experimental evidence obtained using the msbB mutant demonstrates that the blebbing process aids in matrix formation, stabilizing the gonococcal biofilm structure. Autolysis is also known to occur in N. gonorrhoeae [1619]. Membrane from the lysed organisms as well as intracellular contents, such as nucleic acids, may aid in matrix formation. Nucleic acids are known to contribute to biofilm matrix in P. aeruginosa [4].

Figure 1
Biofilm images of Neisseria gonorrhoeae and Neisseria meningitidis depicting a membraneous biofilm matrix

Research is underway to learn more about the gonococcal biofilm environment. Mutational analyses demonstrate that the manganese and zinc transport system, MntABC, is needed to protect the organism against oxidative stress in biofilms grown on glass in flow cells [20]. Further analyses found that mutants lacking oxyR (global regulator of redox response), prx (peroxiredoxin/glutaredoxin), gor (glutathione oxidoreductase) and trxB (thioredoxin reductase) are also deficient in biofilm formation [21,22]. This further emphasizes that neutralization of reactive oxygen and nitrogen species is important in gonococcal biofilm formation. It is unknown at this time if defense from oxidative stress is important in biofilm formation of N. meningitidis.

N. meningtidis biofilms

Carriage is characterized by the presence of meningococcus in the nasopharynx, an antibody response to the carriage strain and the absence of active meningococcal disease [23,24]. In the USA, 5–10% of the civilian population are carriers [25]. In studies of the civilian population, encapsulated meningococci are isolated from carriers up to 86% of the time and average carriage length is reported to be 9.6 months [25]. The ability of a carrier to pass the carriage strain to close contacts varies from 8–50% in studies [25,26]. This wide range in transmission efficiency may be caused by differences in strain characteristics or in carrier behaviors [27]. A stable biofilm population may explain long-term carriage, the typical humoral response against the carriage strain, as well as provide a population to aid in aerosol transmission [25,28].

A multitude of factors are likely to trigger the transition to meningococcal disease from the normal carriage state. Carriage of N. meningitidis and the development of a protective antibody response decreases the likelihood of later disease onset by a different strain [29]. In a survey of three companies of military recruits, five out of 13 soldiers who had no bactericidal antibodies to serogroup C meningococci at the beginning of basic training developed invasive disease from serogroup C N. meningitidis during training, while no subject with high bactericidal antibody titers prior to training developed disease [28]. Development of meningococcal disease occurs within 1–14 days of acquisition of a new strain while carriers of meningococci develop a protective antibody response to the organism 9–10 days following infection [23,30]. Bactericidal antibodies developed to a particular strain also have bactericidal properties to some strains of other serogroups [29]. There is evidence that a respiratory tract infection 7–10 days prior to acquisition of a new N. meningitidis strain in the nasopharynx increases the chances of developing meningococcal disease [23,31]. However, the enhanced possibility of disease with coinfection is more pronounced in adults than in children [31]. These seminal studies in military recruits and civilian populations demonstrate the importance of carriage to prevent active meningococcal disease through the development of a protective antibody response. Chronic infection or carriage is commonly associated with a biofilm mode of growth. Studies that suggest N. meningitidis has the ability to form biofilms in vivo and in vitro are described below.

Clinical evidence of N. meningitidis biofilms in the carrier state

Clinical evidence of meningococcal biofilms during carriage is limited. A comprehensive study of tissue excised during tonsilectomy, adenoidectomy or in surgery to repair sinus passages would be beneficial. A small-scale study was performed that used nasopharyngeal swabs to identify carriers of N. meningitidis in 32 patients who were to have their tonsils removed. This method revealed that 10% of patients were carriers. However, immunolabeling for the PorA protein of the meningococcus on 5 μm frozen sections of the tonsils revealed that 45% of the patients had the meningococcus in their tonsillar tissue [32]. Interestingly, the labeled bacteria appear to be in microcolonies just below the epithelial surface, which could explain why as few as 10% were identified by nasopharyngeal swab. The finding of microcolonies just under the epithelial surface is interesting considering that streptococci can attach to damaged heart valves and form biofilms below the fibrin matrix [33]. It is possible that N. meningitidis can form biofilms in deeper tissues in a similar manner as a result of damage to respiratory tissue from inflammation caused by coincidental bacterial or viral infection, or environmental stresses, such as smoking. The prevelance of meningococcal carriage is known to be higher in individuals exposed to tobacco smoke or recent respiratory tract infection [23,31,34]. The finding of microcolonies within the tonsillar tissue instead of on the surface also raises the possibility of intracellular bacterial communities or intracellular biofilms, as recently demonstrated for uropathogenic E. coli and K. pneumoniae [35]. Uropathogenic E. coli subverts host defenses by living in these intracellular communities. A recent study of meningococcal biofilms on human bronchial epithelial (HBE) cells demonstrates the possibility of meningococci living within the HBE cells at 48 h postinfection [36]. It is possible that N. meningitidis could live in intracellular communities as well, which would allow for persistence and immune evasion [32]. Sim et al. noted that N. meningitidis has homologs to genes of Legionella pneumophilia that are important to the intracellular survival of Legionella [32].

Device-related Neisseria biofilms

Bacteria commonly colonize prosthetics and implant-related devices. The bacteria live on these implants in biofilms and the infection can jeopardize the prognosis of the patient. N. gonorrhoeae can colonize intrauterine devices in a mixed biofilm with other bacteria as described previously [14]. Laryngotracheal stents are often colonized with bacteria after implantation and the bacteria grow in biofilms on the surface of the stent. A clinical study examined 21 patients who had an average age of 37 months for biofilm formation on laryngotracheal stents. All stents were positive for 2–5 different bacterial organisms and 52% were Neisseria. No effort was made to establish if these bacteria were N. meningitidis, N. lactamica or one of the oral Neisseria [37].

Clinical evidence of N. meningitidis biofilms in overt disease

Biofilms are commonly observed in chronic infections. However, recent clinical evidence of meningococcal biofilms in overt disease has been described. Purpura fulminans is a disease state associated with meningococcal sepsis, in which cutaneous, hemorrhagic lesions occur. Immunolabeled skin biopsies have been taken from these lesions to determine if capsule, pili and PorA are expressed during septic infection. All three virulence factors are expressed and interestingly the bacteria are mostly grouped in microcolonies in these lesions [38]. It is unclear if capsule, pili and PorA are important in the formation of the microcolony structure in vivo, or if they are important for other aspects of the disease state. This study indicates the possibility of biofilm formation during symptomatic disease and not just chronic nasopharyngeal infection, however, more work needs to be performed to establish if the presence of microcolonies allows for the progression to mature biofilms in vivo.

In another study of symptomatic meningococcal sepsis, histological sections demonstrate microcolonies of meningococci in brain capillaries, which are likely to have a low blood flow [39]. Further in vitro studies show that meningococci cannot attach to surfaces at high flow rates, however, attachment is achieved at low flow rates. Once attached the bacteria can withstand higher shear forces. In situ imaging of rat brain capillaries demonstrates that meningococci can attach when blood flow temporarily decreases and can then multiply into microcolony-like structures in these capillaries [39]. The studies of brain tissue and purpura fulminans demonstrate the ability of meningococci to form small biofilms in vivo during septic infection [38,39]. However, none of the above studies provide high resolution images that would allow us to determine if a matrix is present in these microcolonies and if the matrix is composed of membranes as established for gonococcal biofilms in vivo [15].

In vitro study of N. meningitidis biofilms Pilus

The role of pilus in meningococcal biofilms has been established on glass. Two studies demonstrate that pilus is important for twitching motility, resulting in the aggregation of meningococci into microcolonies and aiding in 3D architecture of the biofilm [40,41]. A pilus-associated protein (PilX) is responsible for autoaggregation and plays a role in twitching of Neisseria [42]. Meningococcal mutants of pilE, (which encodes the main pilus subunit), or pilX, still form biofilms on glass but have a flat architecture [40]. This indicates that the pilus is not necessary for biofilm formation on glass. Currently, it is not known if the pilus has a role in biofilm formation on human tissue other than its established role as the initial adhesin for pathogenic Neisseria [43].

Capsule

Static biofilm assays in a 96-well polystyrene plate demonstrates that encapsulated meningococci are deficient in biofilm formation, however, a mutant deficient in capsule or a lipooligosaccharide-truncation mutant has an increased biofilm mass and height compared with the wild-type strain [41]. A study that utilized flow cells also demonstrates that encapsulated meningococci are impaired for biofilm formation [40]. These studies suggest that there is a need for hydrophobic interactions to allow for biofilm formation and that the hydrophilic capsule and possibly lipooligosaccharide, block this interaction. Greiner et al. postulate that hydrophobic interactions may be important to Neisserial biofilm formation in a study of N. gonorrhoeae biofilms after demonstration of extensive membraneous material in the biofilm matrix [13].

The finding that encapsulated meningococci do not form biofilms is paradoxical. If biofilms are present in vivo and the organisms do not express capsule, then why would meningococcal capsular conjugate vaccines affect carriage as demonstrated in the UK [44]? It is important to demonstrate the ability of encapsulated N. meningitidis to form biofilms on tissues in order to explain what is known about long-term meningococcal carriage, evasion of innate immune defenses and active disease [38,45,46]. To address this question, a modified flow cell that accommodates a coverslip with a monolayer of transformed airway epithelial cells was used to establish if encapsulated meningococci can form biofilms and to identify bacterial factors involved in biofilm formation. These studies found that encapsulated meningococci can form mature biofilms on SV-40 transformed HBE cells in the flow cell by 48 h. These biofilms had significantly more biomass and a taller average height than biofilms grown on collagen-coated coverslips or on glass alone in the same chambers. In situ immunolabeling of the biofilms as well as ELISA of biofilm material against the meningococcal capsule demonstrate that organisms within the biofilm are encapsulated [36]. This is important because capsule production is phase variable, as well as being regulated by CrgA [47,48]. Unencapsulated N. meningitidis bind to tissue better than encapsulated meningococci [45]. If the only organisms that were phase-off for capsule production bound the HBE cells, then it would be possible that the majority of the organisms that produced the biofilm would also be phase-off. Since capsule production is regulated, it is also possible that organisms in a biofilm environment have capsule production downregulated. The studies on transformed respiratory epithelia demonstrate that the majority of meningococci in the biofilms are encapsulated, showing that phase variation and regulation do not have a major role in capsule production of organisms at the 48 h biofilm time point. Furthermore the average biofilm height of wild-type and isogenic unencapsulated mutants were statistically indistinguishable at 48 h on HBE cells. These studies demonstrate the need for a proper substrate for the meningococci to adhere to and form biofilms. This finding is significant as meningococcal infection, as a biofilm of encapsulated organisms, would make a population of bacteria fitter than unencapsulated organisms as they would be more able to evade host-immune clearance as well as cross the epithelial or endothelial cell layer [45,49].

Two-partner secretion

Two-partner secretion (TPS) is important for biofilm formation in Bordetella bronchiseptica [50]. The secreted member of the TPS system of B. bronchiseptica, filamentous hemagglutinin (FHA), enhances static biofilm formation on 96-well microtiter plates by enhancing attachment to the plate surface [50]. The two-component regulatory system (BvgAS), which regulates FHA production in Bordetella pertussis and B. bronchiseptica, also enhances biofilm formation on glass when the BvgAS system is turned on and inhibits biofilm formation when turned off [51]. This BvgAS-enhanced biofilm formation corresponds to the conditions in which BvgAS induces FHA production. Studies of the N. meningitidis TPS system demonstrate that the secreted TPS member, HrpA, enhances biofilm formation in flow cells on transformed airway epithelial cells [52]. This was the first study of N. meningitidis biofilms to demonstrate a factor involved in the evolution of the biofilm structure on a relevant substrate. HrpA is implicated in different studies in cell association at 5 h following infection, as well as intracellular escape from vacuoles at 7 h following infection [53,54]. Biofilms at the 6 h time point on transformed airway epithelial cells show no difference in biomass between wild-type, mutant or complemented strains. This indicates that differences in initial cell association were not a factor at the 6 h time point, further implicating HrpA as an adhesin. Biofilms grown on collagen-coated coverslips for 48 h also demonstrate reduced biofilm biomass and average height in the hrpA mutant, which shows that egress from the intracellular environment is not a major contributor to the biofilm and not the cause for the hrpA biofilm-associated phenotype. These findings also demonstrate that HrpA has a different role in biofilm formation for N. meningitidis than FHA has for B. bronchiseptica.

The exact function of HrpA within the biofilm is not yet understood, but HrpA processing from a 220 kDa form to a 180 kDa form is enhanced in anaerobic conditions [52]. The oxygen gradient that occurs in large biofilms would produce an environment in which the processed HrpA would be predominant in the deeper recesses of the biofilm. This processed HrpA may have a role in holding the structure of the biofilm together, presumably through bacteria–bacteria interactions. The oxygen gradient may be key to the production of active HrpA and formation of large mature biofilms, as observed in smaller biofilms in the hrpA mutant strains [52]. It is interesting to note that N. gonorrhoeae lacks a functional HrpA and yet, is shown to grow biofilms in vivo, further demonstrating that biofilm formation by the pathogenic Neisseria is multifaceted and not dependent on a single factor.

Tissue destruction in meningococcal biofilms

In the flow-cell system that accommodates airway epithelia, 20% of the cells had perished by 48 h in uninfected flow cells, while 30–40% of the cells were dead in infected flow cells [36]. This may be due to suboptimal media composition or other environmental factors. There is little evidence for tissue destruction in vivo on nasopharyngeal tissue during asymptomatic meningococcal carriage. It is possible that the sums of the innate and adaptive immune defenses force the meningococci into a quiescent biofilm phenotype in vivo and this results in carriage. The flow-cell system lacks components of the innate immune system including complement and professional phagocytes, and lacks all components of the adaptive immune system. This may allow for some of the meningococci to persist with a virulent phenotype in the flow-cell biofilm system. As stated previously, 20% of uninfected airway epithelial cells died in uninfected flow cells within 48 h [36]. This raises the possibility that the airway epithelial cells were in poor health due to flow-cell conditions and the infection enhanced the cell death process that had already begun. Another possibility explaining the enhanced tissue destruction in the biofilm studies is that the meningococcal isolates used in this study were from symptomatic infections and may be more cytotoxic than carrier strains.

While tissue destruction is not known to occur in the carrier state, which we believe to be a biofilm, tissue damage does occur in overt disease. One possible factor that could alter the course of meningococcal infection from a carrier state to an infectious state could be coinfection with another respiratory pathogen. Previous studies link acute respiratory disease from adenovirus, parainfluenza, respiratory syncitial virus, rhinovirus, Mycoplasma species and influenza virus to meningococcal disease [23,31,55,56]. It is unclear if the concurrent infection aids N. meningitidis infection through tissue damage or through suppression of the immune system. As discussed earlier, meningococcal infection is more common in individuals exposed to cigarette smoke [34]. This is a factor that would also damage respiratory epithelia and possibly allow meningococci to take advantage of a weakened mucosal barrier to allow for colonization or disease.

Conclusion

Biofilm communities composed of encapsulated meningococci offer protection from innate host defenses, such as cationic antimicrobial peptides, as well as complement in the nasopharynx, and could provide a reservoir for perpetuating the infection process through aerosolization [45,57]. Histological studies, demonstrating the presence of meningococci in microcolonies on tonsillar tissue, indicate that a biofilm phenotype may be important to carriage. In vitro studies demonstrate that encapsulated and unencapsulated organisms can form biofilms on transformed airway epithelial cells and that capsule and HrpA are important to the composition of the biofilm community. The majority of carrier strains are encapsulated, however, some unencapsulated carrier strains do exist [58]. These are important advances in understanding how meningococci may behave in vivo in a carrier state. The histological study of purpura fulminans biopsies and brain vasculature indicate that microcolonies develop in these tissues during overt disease and that capsule, pilus and PorA are expressed during this process [38,39]. This knowledge of biofilm formation by N. meningitidis is critical since researchers are targeting meningococcal antigens for a N. meningitidis vaccine that is effective against all serogroups of meningococci. It is important that vaccine researchers mimic the natural environment of the host in order to determine which antigens are produced during different phases of infection. Currently, meningococcal biofilm research demonstrates the possibility that one phase of the infection cycle of N. meningitidis is persistence within a biofilm and therefore, has relevance to vaccine research.

The human host is the sole reservoir for N. meningitidis. As such, the bacterium has developed a lifestyle that makes it capable of persisting within the human host and gives it the ability to easily transmit between human carriers. The biofilm mode of growth offers a lifestyle congruent with the notion of long-term carriage and evasion of host immune clearance. The biofilm structure may also be relatively resistant to the innate immune response as characterized by asymptomatic carriage in the nasopharynx of the host for N. meningitidis and in the female for N. gonorrhoeae. The biofilm mode of growth for resistance to oxidative stress is already established for N. gonorrhoeae and could also have a role in meningococcal biofilms [2022]. The presence of encapsulated organisms in the biofilm of a carrier would provide supportive, although not conclusive, evidence of why meningococcal capsular conjugate vaccines are efficacious [44]. Further research as to how the biofilm affects antibiotic treatment options and which antigenic epitopes are present on biofilms is warranted to enhance future treatment of meningococcal disease and the development of vaccines.

Future perspective

Biofilm research with encapsulated N. meningitidis has demonstrated its ability to form biofilms on transformed human respiratory epithelia. This fact should lead to two sets of investigations. The first is to establish whether or not meningococcal biofilms occur in vivo. We believe the biofilm lifestyle is most likely the carrier state of the organism and further work is required to determine the nature of the biofilm in this environment, as well as which antigens are expressed on the surface of the biofilm in order to direct vaccine research. The second set of investigations should be on the immune response to these biofilms. The presence of meningococcal biofilms in the carrier state, composed of capsule-expressing organisms, may explain the efficacy of capsular conjugate vaccines. It is important to understand the interactions of complement, immunoglobulins and sentinel immune cells to developing, as well as established meningococcal biofilms. A minimal or inefficient response by these immune systems could explain the average carriage state of 9.6 months for this organism. However, if one type of immune response is more efficient than another, those findings could help direct future therapy against this organism. It would also be important to determine if all capsular serotypes have the ability to form biofilms and if strains with low invasive potential have increased or decreased ability to form biofilms compared with epidemic strains.

Executive summary

Bacterial biofilms

  • Biofilms are formed under conditions of environmental stress, which affords microbes more protection from environmental factors than if they were in an individual planktonic state.

Biofilm formation by pathogenic Neisseria

  • Neisseria gonorrhoeae forms biofilms in vivo and in vitro. The oxidative stress-response pathways are essential to this process. The oral Neisseria also form biofilms on the dental surface.

Clinical evidence of Neisseria meningitidis biofilms in the carrier state

  • Histological sections of tonsillar tissue demonstrate microcolony-like structures of meningococci within the tissues. Further research is needed to determine if these structures are enveloped within a matrix, which would define them as a biofilm.

Device-related Neisseria biofilms

  • Laryngotracheal stents are often colonized with multispecies biofilms that include the Neisseria genera. It is unclear at this time which of the oral or nasopharyngeal Neisseria is responsible for this colonization.

Clinical evidence for Neisseria meningitidis biofilms in overt disease

  • Microcolony-like structures of Neisseria meningitidis are observed in sections of brain tissue and in biopsies from purpura fulminans. It is unclear at this time if these structures matured to the state of developed biofilms by becoming enveloped within a matrix.

In vitro study of Neisseria meningitidis biofilms

  • Pilus is essential for the 3D architecture of the meningococcal biofilm on glass in flow cells. Mutations in pilE or pilX result in flat biofilms.
  • Capsule inhibits biofilm formation by N. meningitidis on plastic and glass. However, capsule does not inhibit biofilm formation on transformed human respiratory epithelia. This may have implications on the efficacy of capsular conjugate vaccines if encapsulated organisms form biofilms in the carrier state.
  • Two-partner secretion contributes to biofilm formation on transformed human respiratory tissue through the secretion and deposition of HrpA on the surface of the bacterium. HrpA is thought to stabilize the architecture of the biofilm with the processed form of the HrpA protein. This processed form is most prevalent in environments of low oxygen, as may be the case within the middle of the biofilms.

Tissue destruction in meningococcal biofilms

  • N. meningitidis biofilms on transformed human respiratory tissue in flow cells resulted in increased tissue destruction when compared with tissue in uninfected flow cells. Tissue destruction by N. meningitidis has also been seen in infection of nasopharyngeal organ culture. Further investigation would help determine if suboptimal media composition contributed to this effect or if this is a mechanism that contributes to invasive disease.

Conclusion

  • Meningococci have the ability to form mature biofilms in vitro.
  • More work is needed to determine if mature meningococcal biofilms form in vivo.
  • Future research may result in better vaccine candidates and a better understanding of the immune response to meningococcal biofilms.

Acknowledgments

Financial & competing interests disclosure

The work in this manuscript has been supported by the National Institute of Allergy and Infectious Diseases (NIAID) grant AI AI045728. The authors have noother relevant affiliations or financial involvement with any organization or entity with a financial interest in or financial conflict with the subject matter or materials discussed in the manuscript apart from those disclosed.

No writing assistance was utilized in the production of this manuscript.

Footnotes

For reprint orders, please contact: moc.enicidemerutuf@stnirper

Contributor Information

R Brock Neil, University of Iowa, Hygienic Laboratory, 102 Oakdale Campus, H101 OH, Iowa City, IA 52242-5002, USA, Tel.: +1 319 335 4380; Fax: +1 319 335 4555.

Michael A Apicella, Department of Microbiology, 3–401 BSB, University of Iowa, Iowa City, IA 52242, USA, Tel.: +1 319 335 7807; Fax: +1 319 335 9006.

Bibliography

Papers of special note have been highlighted as:

[filled square] of interest

[filled square][filled square] of considerable interest

1[filled square]. Hall-Stoodley L, Costerton JW, Stoodley P. Bacterial biofilms: from the natural environment to infectious diseases. Nat Rev Microbiol. 2004;2(2):95–108. Excellent review of general aspects of biofilm formation by bacteria. [PubMed]
2. Anderson GG, O’Toole GA. Innate and induced resistance mechanisms of bacterial biofilms. Curr Top Microbiol Immunol. 2008;322:85–105. [PubMed]
3. Hausner M, Wuertz S. High rates of conjugation in bacterial biofilms as determined by quantitative in situ analysis. Appl Environ Microbiol. 1999;65(8):3710–3713. [PMC free article] [PubMed]
4. Mulcahy H, Charron-Mazenod L, Lewenza S. Extracellular DNA chelates cations and induces antibiotic resistance in Pseudomonas aeruginosa biofilms. PLoS Pathog. 2008;4(11):e1000213. [PMC free article] [PubMed]
5. Smyth A. Update on treatment of pulmonary exacerbations in cystic fibrosis. Curr Opin Pulm Med. 2006;12(6):440–444. [PubMed]
6. Starner TD, Zhang N, Kim G, Apicella MA, McCray PB., Jr Haemophilus influenzae forms biofilms on airway epithelia: implications in cystic fibrosis. Am J Respir Crit Care Med. 2006;174(2):213–220. [PMC free article] [PubMed]
7. Murphy TF. Respiratory infections caused by nontypeable Haemophilus influenzae. Curr Opin Infect Dis. 2003;16(2):129–134. [PubMed]
8. Donlan RM, Costerton JW. Biofilms: survival mechanisms of clinically relevant microorganisms. Clin Microbiol Rev. 2002;15(2):167–193. [PMC free article] [PubMed]
9. Stickler DJ. Bacterial biofilms in patients with indwelling urinary catheters. Nat Clin Pract Urol. 2008;5(11):598–608. [PubMed]
10. Ala’Aldeen DA, Neal KR, Ait-Tahar K, et al. Dynamics of meningococcal long-term carriage among university students and their implications for mass vaccination. J Clin Microbiol. 2000;38(6):2311–2316. [PMC free article] [PubMed]
11. Bennett JS, Griffiths DT, McCarthy ND, et al. Genetic diversity and carriage dynamics of Neisseria lactamica in infants. Infect Immun. 2005;73(4):2424–2432. [PMC free article] [PubMed]
12. Handsfield HH, Sparling PF. Principles and Practice of Infectious Diseases. Vol. 2. Churchill Livingstone; New York, NY, USA: 2005. Neisseria gonorrhoeae; pp. 2514–2529.
13. Greiner LL, Edwards JL, Shao J, et al. Biofilm formation by Neisseria gonorrhoeae. Infect Immun. 2005;73(4):1964–1970. [PMC free article] [PubMed]
14. Pruthi V, Al-Janabi A, Pereira BJ. Characterization of biofilm formed on intrauterine devices. Indian J Med Microbiol. 2003;21(3):161–165. [PubMed]
15[filled square][filled square]. Steichen CT, Shao JQ, Ketterer MR, Apicella MA. Gonococcal cervicitis: a role for biofilm in pathogenesis. J Infect Dis. 2008;198(12):1856–1861. Demonstrates the ability of Neisseria gonorrhoeae to form biofilms in vivo on cervical biopsie. [PMC free article] [PubMed]
16. Bos MP, Tefsen B, Voet P, et al. Function of Neisserial outer membrane phospholipase A in autolysis and assessment of its vaccine potential. Infect Immun. 2005;73(4):2222–2231. [PMC free article] [PubMed]
17. Dillard JP, Seifert HS. A peptidoglycan hydrolase similar to bacteriophage endolysins acts as an autolysin in Neisseria gonorrhoeae. Mol Microbiol. 1997;25(5):893–901. [PubMed]
18. Garcia DL, Dillard JP. AmiC functions as an N-acetylmuramyl-L-alanine amidase necessary for cell separation and can promote autolysis in Neisseria gonorrhoeae. J Bacteriol. 2006;188(20):7211–7221. [PMC free article] [PubMed]
19. Garcia DL, Dillard JP. Mutations in ampG or ampD affect peptidoglycan fragment release from Neisseria gonorrhoeae. J Bacteriol. 2008;190(11):3799–3807. [PMC free article] [PubMed]
20. Lim KH, Jones CE, vanden Hoven RN, et al. Metal binding specificity of the MntABC permease of Neisseria gonorrhoeae and its influence on bacterial growth and interaction with cervical epithelial cells. Infect Immun. 2008;76(8):3569–3576. [PMC free article] [PubMed]
21. Potter AJ, Kidd SP, Edwards JL, et al. Thioredoxin reductase is essential for protection of Neisseria gonorrhoeae against killing by nitric oxide and for bacterial growth during interaction with cervical epithelial cells. J Infect Dis. 2009;199(2):227–235. [PMC free article] [PubMed]
22. Seib KL, Wu HJ, Srikhanta YN, et al. Characterization of the OxyR regulon of Neisseria gonorrhoeae. Mol Microbiol. 2007;63(1):54–68. [PubMed]
23. Edwards EA, Devine LF, Sengbusch GH, Ward HW. Immunological investigations of meningococcal disease III Brevity of group C acquisition prior to disease occurrence. Scand J Infect Dis. 1977;9(2):105–110. [PubMed]
24. Caugant DA, Tzanakaki G, Kriz P. Lessons from meningococcal carriage studies. FEMS Microbiol Rev. 2007;31(1):52–63. [PubMed]
25. Greenfield S, Sheehe PR, Feldman HA. Meningococcal carriage in a population of “normal” families. J Infect Dis. 1971;123(1):67–73. [PubMed]
26. Wilder-Smith A, Barkham TMS, Ravindran S, Earnest A, Paton NI. Persistence of W135 Neisseria meningitidis carriage in returning Hajj pilgrims: risk for early and late transmission to household contacts. Emerg Infect Dis. 2003;9(1):123–126. [PMC free article] [PubMed]
27. Broome CV. The carrier state: Neisseria meningitidis. J Antimicrob Chemother. 1986;18(Suppl A):25–34. [PubMed]
28. Goldschneider I, Gotschlich EC, Artenstein MS. Human immunity to the meningococcus I The role of humoral antibodies. J Exp Med. 1969;129(6):1307–1326. [PMC free article] [PubMed]
29. Reller LB, MacGregor RR, Beaty HN. Bactericidal antibody after colonization with Neisseria meningitidis. J Infect Dis. 1973;127(1):56–62. [PubMed]
30. Tzeng YL, Stephens DS. Epidemiology and pathogenesis of Neisseria meningitidis. Microbes Infect. 2000;2(6):687–700. [PubMed]
31. Moore PS, Hierholzer J, DeWitt W, et al. Respiratory viruses and mycoplasma as cofactors for epidemic group A meningococcal meningitis. JAMA. 1990;264(10):1271–1275. [PubMed]
32. Sim RJ, Harrison MM, Moxon ER, Tang CM. Underestimation of meningococci in tonsillar tissue by nasopharyngeal swabbing. Lancet. 2000;356(9242):1653–1654. [PubMed]
33. Parsek MR, Singh PK. Bacterial biofilms: an emerging link to disease pathogenesis. Annu Rev Microbiol. 2003;57:677–701. [PubMed]
34. MacLennan J, Kafatos G, Neal K, et al. Social behavior and meningococcal carriage in British teenagers. Emerg Infect Dis. 2006;12(6):950–957. [PMC free article] [PubMed]
35. Rosen DA, Pinkner JS, Jones JM, et al. Utilization of an intracellular bacterial community pathway in Klebsiella pneumoniae urinary tract infection and the effects of FimK on type 1 pilus expression. Infect Immun. 2008;76(7):3337–3345. [PMC free article] [PubMed]
36[filled square]. Neil RB, Shao J, Apicella MA. Biofilm formation on human airway epithelia by encapsulated Neisseria meningitidis serogroup B. Microbes Infect. 2009;11(2):281–287. First demonstration of meningococcal biofilms on human tissue and demonstrates capsule does not inhibit biofilm formation on tissue. [PubMed]
37. Simoni P, Wiatrak BJ. Microbiology of stents in laryngotracheal reconstruction. Laryngoscope. 2004;114(2):364–367. [PubMed]
38. Harrison OB, Robertson BD, Faust SN, et al. Analysis of pathogen–host cell interactions in purpura fulminans: expression of capsule, type IV pili, and PorA by Neisseria meningitidis in vivo. Infect Immun. 2002;70(9):5193–5201. [PMC free article] [PubMed]
39[filled square]. Mairey E, Genovesio A, Donnadieu E, et al. Cerebral microcirculation shear stress levels determine Neisseria meningitidis attachment sites along the blood–brain barrier. J Exp Med. 2006;203(8):1939–1950. Excellent modeling of Neisseria meningitidis attachment to tissue under shear stress. [PMC free article] [PubMed]
40[filled square]. Lappann M, Haagensen JA, Claus H, Vogel U, Molin S. Meningococcal biofilm formation: structure, development and phenotypes in a standardized continuous flow system. Mol Microbiol. 2006;62(5):1292–1309. Demonstration that pili are important to the architecture of N. meningitidis biofilms in a glass flow cell. [PubMed]
41. Yi K, Rasmussen AW, Gudlavalleti SK, Stephens DS, Stojiljkovic I. Biofilm formation by Neisseria meningitidis. Infect Immun. 2004;72(10):6132–6138. [PMC free article] [PubMed]
42. Helaine S, Carbonnelle E, Prouvensier L, et al. PilX, a pilus-associated protein essential for bacterial aggregation, is a key to pilus-facilitated attachment of Neisseria meningitidis to human cells. Mol Microbiol. 2005;55(1):65–77. [PubMed]
43. Rudel T, Scheurerpflug I, Meyer TF. Neisseria PilC protein identified as type-4 pilus tip-located adhesin. Nature. 1995;373(6512):357–359. [PubMed]
44. Maiden MC, Ibarz-Pavon AB, Urwin R, et al. Impact of meningococcal serogroup C conjugate vaccines on carriage and herd immunity. J Infect Dis. 2008;197(5):737–743. [PubMed]
45[filled square]. Spinosa MR, Progida C, Tala A, et al. The Neisseria meningitidis capsule is important for intracellular survival in human cells. Infect Immun. 2007;75(7):3594–3603. Important demonstration that the meningococcal capsule is important for intracellular environment survival. [PMC free article] [PubMed]
46. Vogel U, Weinberger A, Frank R, et al. Complement factor C3 deposition and serum resistance in isogenic capsule and lipooligosaccharide sialic acid mutants of serogroup B Neisseria meningitidis. Infect Immun. 1997;65(10):4022–4029. [PMC free article] [PubMed]
47. Deghmane A-E, Giorgini D, Larribe M, Alonso J-M, Taha M-K. Down-regulation of pili and capsule of Neisseria meningitidis upon contact with epithelial cells is mediated by CrgA regulatory protein. Mol Microbiol. 2002;43(6):1555–1564. [PubMed]
48. Lavitola A, Bucci C, Salvatore P, et al. Intracistronic transcription termination in polysialyltransferase gene (siaD) affects phase variation in Neisseria meningitidis. Mol Microbiol. 1999;33(1):119–127. [PubMed]
49. Nikulin J, Panzner U, Frosch M, Schubert-Unkmeir A. Intracellular survival and replication of Neisseria meningitidis in human brain microvascular endothelial cells. Int J Med Microbiol. 2006;296(8):553–558. [PubMed]
50. Irie Y, Mattoo S, Yuk MH. The Bvg virulence control system regulates biofilm formation in Bordetella bronchiseptica. J Bacteriol. 2004;186(17):5692–5698. [PMC free article] [PubMed]
51. Mishra M, Parise G, Jackson KD, Wozniak DJ, Deora R. The BvgAS signal transduction system regulates biofilm development in Bordetella. J Bacteriol. 2005;187(4):1474–1484. [PMC free article] [PubMed]
52. Neil RB, Apicella MA. Role of HrpA in biofilm formation of Neisseria meningitidis and regulation of the hrpBAS transcript. Infect Immun. 2009 doi: 10.1128/IAI.01502-08. (Epub ahead of print) [PMC free article] [PubMed] [Cross Ref]
53. Schmitt C, Turner D, Boesl M, et al. A functional two-partner secretion system contributes to adhesion of Neisseria meningitidis to epithelial cells. J Bacteriol. 2007;189(22):7968–7976. [PMC free article] [PubMed]
54. Tala A, Progida C, De Stefano M, et al. The HrpB–HrpA two-partner secretion system is essential for intracellular survival of Neisseria meningitidis. Cell Microbiol. 2008;10(12):2461–2482. [PubMed]
55. Eickhoff TC. Sero-epidemiologic studies of meningococcal infection with the direct hemagglutination test. J Infect Dis. 1971;123(5):519–526. [PubMed]
56. Young LS, LaForce FM, Head JJ, Feeley JC, Bennett JV. A simultaneous outbreak of meningococcal and influenza infections. N Engl J Med. 1972;287(1):5–9. [PubMed]
57. Ooi EH, Wormald PJ, Tan LW. Innate immunity in the paranasal sinuses: a review of nasal host defenses. Am J Rhinol. 2008;22(1):13–19. [PubMed]
58. Cartwright KA, Stuart JM, Jones DM, Noah ND. The Stonehouse Survey: nasopharyngeal carriage of meningococci and Neisseria lactamica. Epidemiol Infect. 1987;99(3):591–601. [PMC free article] [PubMed]