Skip to main content
  • Loading metrics

Thermoregulation of Meningococcal fHbp, an Important Virulence Factor and Vaccine Antigen, Is Mediated by Anti-ribosomal Binding Site Sequences in the Open Reading Frame

  • Edmund Loh,

    Current address: Department of MTC, Mikrobiell Patogenes, Gustaf V:s Forskningsinstitut Karolinska Instituet, Stockholm, Sweden

    Affiliation Sir William Dunn School of Pathology, University of Oxford, Oxford, United Kingdom

  • Hayley Lavender,

    Affiliation Sir William Dunn School of Pathology, University of Oxford, Oxford, United Kingdom

  • Felicia Tan,

    Affiliation Sir William Dunn School of Pathology, University of Oxford, Oxford, United Kingdom

  • Alexander Tracy,

    Affiliation Sir William Dunn School of Pathology, University of Oxford, Oxford, United Kingdom

  • Christoph M. Tang

    Affiliation Sir William Dunn School of Pathology, University of Oxford, Oxford, United Kingdom


During colonisation of the upper respiratory tract, bacteria are exposed to gradients of temperatures. Neisseria meningitidis is often present in the nasopharynx of healthy individuals, yet can occasionally cause severe disseminated disease. The meningococcus can evade the human complement system using a range of strategies that include recruitment of the negative complement regulator, factor H (CFH) via factor H binding protein (fHbp). We have shown previously that fHbp levels are influenced by the ambient temperature, with more fHbp produced at higher temperatures (i.e. at 37°C compared with 30°C). Here we further characterise the mechanisms underlying thermoregulation of fHbp, which occurs gradually over a physiologically relevant range of temperatures. We show that fHbp thermoregulation is not dependent on the promoters governing transcription of the bi- or mono-cistronic fHbp mRNA, or on meningococcal specific transcription factors. Instead, fHbp thermoregulation requires sequences located in the translated region of the mono-cistronic fHbp mRNA. Site-directed mutagenesis demonstrated that two anti-ribosomal binding sequences within the coding region of the fHbp transcript are involved in fHbp thermoregulation. Our results shed further light on mechanisms underlying the control of the production of this important virulence factor and vaccine antigen.

Author Summary

The bacterium Neisseria meningitidis is exquisitely adapted to survive in the human host, and possesses several mechanisms to interact with host cells in the upper airway and to circumvent immune responses. However, the mechanisms that govern the expression of factors that contribute to colonisation and disease are incompletely understood. In this work, we further characterise how temperature influences the production of factor H binding protein (fHbp) by the meningococcus; fHbp recruits human complement proteins to the surface of the bacterium, and is an important vaccine antigen. We show that thermoregulation of fHbp occurs gradually over a physiological range of temperatures found in the upper airway, the site of colonisation. This regulation does not require specific meningococcal transcription factors, and sequence analysis indicates that fHbp mRNA forms a secondary structure which could act as an RNA thermosensor. Additional studies demonstrate that there are two specific sequences within the coding region of fHbp mRNA are important for thermosensing and could base-pair to the ribosome binding site, thus blocking translation of this protein. As fHbp is thermoregulated, vaccines that target this antigen might not impose a high level of selective pressure on the bacterium at the mucosal surface, thereby limiting herd immunity induce by fHbp containing vaccines.


Neisseria meningitidis is a harmless member of the human nasopharyngeal flora in a significant proportion of healthy individuals [1]. However in some instances, the bacterium spreads from the upper airway into the systemic circulation, where it can replicate and spread to the rest of the body [2], especially the cerebrospinal fluid, resulting in meningitis. Therefore the meningococcus remains an important human pathogen in infants and young adults [3].

To survive in the human host, the meningococcus has evolved several mechanisms that enable it to evade the immune system [4]. In particular, the complement system is critical for protection against systemic N. meningitidis infection, evident from the increased susceptibility of individuals with defects in the complement system and findings from a genome wide association study [5,6]. The bacterium evades complement mediated killing by expressing a polysaccharide capsule, sialylation of its lipopolysaccharide, and by binding complement factor H (CFH), the major negative regulator of the alternative complement pathway [7]. CFH is recruited by high affinity interactions with factor H binding protein (fHbp) [8]. CFH competes with complement factor H related protein-3 (CFHR3) for binding to fHbp on the meningococcus [9]; CFHR3 is a competitive inhibitor of CFH binding to the meningococcal surface, and relative levels of CFH and CFHR3 in individuals are likely to determine host genetic susceptibility to meningococcal disease in the general population [9]. Furthermore fHbp is a surface lipoprotein which is an important component of two vaccines which are now licensed for preventing meningococcal disease [10,11].

Within the upper airway, the bacterium is exposed to gradients in ambient temperature that occur in relation to the anatomical location the phase in the respiratory cycle, and the presence of local inflammation [12,13]. The nasal epithelium contains a complex vascular network with a relatively high blood flow, which forms a heat exchanger, to condition inspired air; the temperature of air entering the nasopharynx rises rapidly from the nostrils, increasing to around 32–34°C by the time it reaches the glottis at the end of inspiration [14,15]. During colonisation, the meningococcus is found both on the epithelial surface as well as deep in the submucosal layer surface [16], so the bacterium will be will be exposed to a range of temperatures in these sites [17]. Additionally, during the development of invasive disease, N. meningitidis passes from the lower temperatures in the upper airway to the core body temperature of 37°C or higher with a febrile response to infection [18]. Therefore, temperature is likely to be an important environmental cue for the meningococcus during colonisation and the development of disease.

We have shown previously that three meningococcal genes, cssA, fHbp, and lst which encode factors contributing to capsule biosynthesis, fHbp, and LPS sialylation, respectively, are subject to thermoregulation. Of note, the sialic acid-capsule biosynthesis operon is controlled by an RNA thermosensor [19]. RNA thermosensors are usually located in the 5´-untranslated region (5´-UTR) of an mRNA, and form a secondary structure at lower temperatures that prevents protein translation by blocking access of ribosomes to the nascent mRNA. As the temperature rises, the secondary structure undergoes a conformational change, exposing the ribosome binding site (RBS), and allowing translation in response to the elevated temperature. RNA thermosensors have been described in an increasing number of microbes [20], especially enteric pathogens which are subject to a large fluctuation in temperature upon ingestion by mammalian hosts from the external environment.

Here we describe the mechanisms governing thermoregulation of fHbp. Expression of fHbp in N. meningitidis is initiated from two transcriptional start sites, resulting in a bi-cistronic transcript (including the upstream gene, nmb1869), or a mono-cistronic transcript from the fHbp promoter, PfHbp [21]. It has been shown that transcription from PfHbp is responsive to oxygen limitation, and regulated in an FNR-dependent manner [21]. We demonstrate that fHbp levels are governed by an RNA thermosensor and demonstrate that sequences in the coding region of fHbp contribute to thermosensing and translation efficiency; two sequences within the fHbp coding region, which are complementarity to the ribosome-binding site, are necessary for the thermoregulation of this key virulence factor and vaccine antigen.


fHbp expression is temperature-dependent

We have shown previously that levels of fHbp in the meningococcus increase following growth at higher temperatures [19]. To determine whether this affects the level of fHbp on the bacterial surface, we analysed bacteria grown at different temperatures by flow cytometry using αfHbp pAbs (Fig 1A). The results demonstrate that a rise in temperature is associated with a significant increase in the amount of fHbp on the meningococcus between bacteria grown at 30°C and 42°C.

Fig 1. Thermoregulation of fHbp occurs post-transcriptionally.

(A) N. meningitidis MC58 was grown at the temperatures indicated until mid-log, then subjected to flow cytometry analysis using anti- V1.1 fHbp pAbs to detect surface localised fHbp. Representative graph of fHbp detection at indicated temperatures. Secondary antibody only used as a control (grey). Geometric mean fluorescence of surface expressed fHbp from three independent experiments; error bars are ± SEM. Stastically significant levels of fHbp were detected between bacteria grown at 30°C and 42°C. (B) RNA was obtained at mid-log phase from bacteria grown at the temperatures indicated, and samples (20 μg) were separated on agarose-formaldehyde gel and subjected to Northern blot analysis with probes for fHbp and tmRNA. The position of bands corresponding to the mono- and bi-cistronic transcripts are shown. (C) Proteins extracted from the same cultures as in B were analysed by Western blot. Relative levels of RNA and protein are indicated. (D) Western blot analysis of protein stability. Bacteria were grown at 30°C or 37°C until mid-log phase, then protein synthesis blocked by the addition of spectinomycin. Samples were removed at time-points afterwards and subjected Western blot analysis. Membranes were probed with antibodies recognising fHbp or RecA (loading control).

To establish whether this change is mediated by an alteration in the transcription of fHbp, N. meningitidis was grown to mid-log phase at 30°C, 37°C or 42°C, and fHbp mRNA detected by Northern analysis. Of note, levels of the bi- and mono-cistronic transcripts of fHbp mRNA were unaffected by temperature, demonstrated by Northern blot analysis (Fig 1B). However, analysis of samples from the same experiment demonstrate that there was an accompanying clear increase in fHbp levels at higher temperatures (Fig 1C) as described previously [19], indicating that thermal regulation of fHbp occurs at the post-transcriptional level.

To examine whether the increase in fHbp at higher temperatures results from an alteration in protein stability, N. meningitidis was grown at different temperatures to mid-log phase then de novo protein synthesis was inhibited by adding spectinomycin to cultures. Western blot analyses of samples taken at times afterwards demonstrate that there is no detectable difference in the stability of fHbp in N. meningitidis at 30 and 37°C (Fig 1D). Taken together, these results indicate that the thermoregulation of fHbp does not result from a change in transcription or protein degradation.

The promoter of the monocistronic fHbp mRNA is dispensible for thermoregulation

Thermoregulation of fHbp was analysed in Escherichia coli using a plasmid (pfHbp) containing the mono-cistronic fHbp and its promoter, PfHbp (Fig 2A and [19]); results demonstrate that the bi-cistronic mRNA is dispensable for fHbp thermoregulation. To further define the mechanism of thermoregulation, we examined the level of fHbp mRNA in E. coli harbouring pfHbp grown at 30°C, 37°C and 42°C; consistent with results obtained with N. meningitidis, there was no discernible change in transcript levels following growth at different temperatures (Fig 2B), even though fHbp was subject to clear thermoregulation in the same samples (Fig 2C). To identify sequences that contribute to thermoregulation, we generated a plasmid (pfHbpΔPfHbp) that includes the 5´-UTR of the transcript but lacks its native promoter, PfHbp; in this plasmid, transcription of fHbp occurs from the T7 promoter in the vector (Fig 2A) or the SP6 promoter in the opposite orientation. Again a temperature-dependent increase in fHbp levels was observed in E. coli harbouring fHbp in either orientation in this plasmid (Fig 2D and S1 Fig), demonstrating that PfHbp is not required for fHbp thermoregulation. In contrast, deletion of the 5´ UTR from pfHbpΔPfHbp (generating pfHbpΔPfhbpΔUTR) led to loss of fHbp thermoregulation, indicating that the 5´-UTR of the monocistronic fHbp mRNA is required for thermoregulation in this system lacking the bicistronic transcript (Fig 2E).

Fig 2. fHbp thermoregulation requires the 5´-UTR of fHbp mRNA.

(A) Sequence of the insert in pfHbp indicating the sites of T7 and PfHbp promoters (green and blue arrows, respectively), the FNR box (yellow), the PfHbp -35 and -10 sequences with the RBS (shown blue), and the start codon, red, GTG). (B) E. coli containing pfHbp was grown at the temperatures indicated until mid-log, then RNA was extracted and subjected to Northern analysis with probes for fHbp and tmRNA. (C) Protein was obtained from the same samples as for RNA analysis and examined by Western blot using antibodies against fHbp and RecA (as a loading control). (D) E. coli containing a plasmid (pfHbpΔPfHbp, deleted sequences underlined with dashed line in panel A) lacking the FNR box and Pfhbp still demonstrates fHbp thermoregulation. (E) Removal of the 5´-UTR from pfHbpΔPfHbp (generating pfHbpΔPfHbpΔUTR, further deleted sequences underlined with dotted line in panel A) abolishes fHbp thermoregulation.

To examine the relevance of these findings in N. meningitidis, we substituted the open reading frame (ORF) upstream of fHbp (i.e. nmb1869, 1065 bp in length) with the 1120 bp kanamycin resistance marker in N. meningitidis to i) leave the promoter for the bi-cistronic transcript intact, and ii) disrupt Pfhbp promoter (Fig 3A and 3B), generating strain mutPfHbp-10. Northern analysis confirmed loss of the monocistronic fHbp mRNA (Fig 3C), and thermoregulation was still observed in the meningococcus with the bi-cistronic transcript alone (Fig 3D). Together with the findings in E. coli (Fig 2), the results provide evidence that the monocistronic PfHbp is dispensable for fHbp thermoregulation.

Fig 3. PfHbp is dispensable for fHbp thermoregulation in N. meningitidis.

(A, B) A N. meningitidis strain (mut PfHbp-10) was generated in which nmb1869 was replaced with a promoterless kanamycin resistance cassette and the -10 sequence of PfHbp was mutated (nt. changes shown in red); the position of the predicted -35 and -10 sequences of PfHbp are in blue. (C) Northern blot analysis confirmed the absence of the monocistronic fHbp mRNA in N. meningitidis mut PfHbp-10. (D) Bacteria were grown in BHI medium until mid-log phase at indicated temperatures, and western blot analysis was performed with antibodies recognising fHbp or RecA (loading control).

Expression of fHbp is influenced by sequences in the coding region

Next we generated plasmids containing the 5´-UTR with the first one, five or nine codons of fHbp fused to GFP as a reporter (pfHbp1C-gfp, pfHbp5C-gfp and pfHbp9C-gfp, respectively, Fig 4A); we were unable to generate constructs with more codons, probably because of toxic effects of the fHbp leader sequence in E. coli. The plasmids lack a T7 promoter [22], so expression is governed by the native fHbp promoter. We observed a clear correlation between number of fHbp codons in the plasmid and levels of the GFP reporter, with approximately 3.5-fold higher GFP in bacteria harbouring pfHbp9C-gfp compared with fHbp1C-gfp following growth at 37°C (Fig 4B). The increase in GFP levels observed with pfHbp9C-gfp is not caused by a change in protein or RNA stability (S2 Fig), but instead correlates with the predicted minimum free energy values (using the Vienna RNAfold package, Fig 4C) and putative secondary structures (S3 Fig).

Fig 4. Translation of fHbp is enhanced by its initial codons.

(A) Sequence of pfHbp-9C-gfp, a GFP reporter plasmid including nine fHbp codons. The construct includes PfHbp (-10 and -35 indicated, and blue arrow for the TSS) with the 5´-UTR and nine codons of fHbp open as a translational fusion with GFP in pEGFP-N2: PfHbp, blue arrow; blue box denotes the first nine codons of fHbp. (B) Cultures of E. coli containing plasmids harbouring one, five or nine codons, or containing the empty vector pEGFP-N2 were grown at 37°C until mid-log phase. Whole cell lysates were subjected to Western blot analysis with antibodies recognising GFP or RecA (loading control). Relative expression values (indicated). (C) Table of the predicted minimum free energies in kcal/mole (ΔG) of potential secondary RNA structures of sequences introduced into the plasmids (A) with the number of nucleotides shown (nt.).

Gradual thermoregulation of fHbp in an in vitro system

To determine whether thermoregulation of fHbp was also observed in a cell free system, in vitro transcription/translation assays were performed with pfHbp1C-gfp, pfHbp5C-gfp and pfHbp9C-gfp. DNA from these plasmids was transcribed and translated in a continuous manner at 30°C or 37°C, and GFP production assayed by Western blot analysis (Fig 5A). There was increased GFP generated in assays performed at the higher temperature with pfHbp5C-gfp and pfHbp9C-gfp; however thermoregulation was not observed in assays containing pfHbp1C-gfp. Overall levels of GFP produced were higher in assays with plasmids harbouring more codons, consistent with sequences in the ORF enhancing translation efficiency. Therefore, the fHbp9C-GFP construct was used in subsequent experiments.

Fig 5. Gradual thermoregulation of fHbp-GFP.

(A) In vitro transcription/translation assays using DNA from pfHbp-1C-gfp pfHbp-5C-gfp or pfHbp-9C-gfp (number of codons shown above each lane) performed at the indicated temperatures for 1 hr. Samples were subject to Western analysis. (B) Gradual thermoregulation of fHbp-GFP. RNA was isolated from E. coli containing pfHbp-9C-gfp construct was subjected to in vitro translation at indicated temperatures. Western analysis was performed using antibodies recognising GFP or RecA.

To further examine the dynamics of fHbp thermoregulation, in vitro transcription/translation reactions were conducted with pfHbp9C-gfp at temperatures between 30°C and 38°C. Equal amounts of plasmid were used as the substrate for in vitro transcription/translation reactions performed at 30°C, 34°C, 36°C, 37°C and 38°C for one hour, and reaction products were analysed by Western blotting. The results demonstrate that levels of the GFP reporter rise gradually in response to increasing temperature over a physiological range (Fig 5B) similar to the cssA thermosensor [19].

Anti-ribosomal binding site sequences in the fHbp ORF contribute to fHbp thermosensing

Next, we performed mutagenesis to identify key nucleotides involved in the formation of putative RNA secondary structures in the fHbp mRNA that mediate thermoregulation. Several point mutations were introduced upstream of the fHbp GTG start codon in pfHbp9C-gfp (Fig 6A), and their effect examined during growth of E. coli at 30°C, 37°C and 42°C. Proteins were isolated from the bacteria and levels of GFP expression examined by Western blot analysis. However, none of the single base substitutions in the 5´-UTR disrupted thermoregulation (Fig 6B), indicating that these changes are insufficient to perturb RNA secondary structures that are necessary for thermosensing.

Fig 6. Modification of nucleotides in the fHbp 5´-UTR does not abolish thermoregulation.

(A) Predicted RNA secondary structure of the whole 5´-UTR and 34 bases of fHbp-mRNA. (RBS indicated in blue, start codon in red, putative α-RBSs in yellow). The nucleotides modified in pfHbp-9C-gfp are indicated. (B) Western blot analysis of fHbp-GFP levels in E. coli harbouring plasmids with modified fHbp 5´-UTRs. Bacteria were grown to mid-log phase at the indicated temperatures, and whole cell lysates subjected to Western blot analysis with antibodies recognising GFP or RecA. Relative values (rel. values) of GFP are indicated below each lane.

On further inspection, we identified two copies of a 6 bp repeat (CUGCCU) within the fHbp coding region, close to the start codon and potentially able to base-pair with the ribosome binding site (RBS); we termed these repeats αRBS-1 and αRBS-2 (Fig 6A). We reasoned that the two cytosines could base-pair with the guanines in the RBS (AGGAG) and prevent ribosomes binding to the nascent transcript. Therefore, site-directed mutagenesis was performed to modify the two cytosines to guanines in each αRBS (i.e. CUGCCU to CUGGGU) either singly (generating mutαRBS-1 and mutαRBS-2), or together (mutαRBS-1/2). Constructs were introduced into E. coli, which was then grown at 30°C, 37°C and 42°C, and the level of GFP examined by Western blot analysis. All three constructs displayed reduced fHbp thermoregulation when compared to the plasmid containing wild-type sequences. Comparing cultures grown at 30°C or 42°C, the level of GFP increased by 1.5-fold and 1.6-fold for cells harbouring mutαRBS-1 and mutαRBS-2, respectively, whereas cells containing mutαRBS-1/2, showed a 1.2-fold increase (Fig 7A). In contrast, GFP levels increased by 5.3-fold with the wild-type sequence in the plasmid. RecA levels were stable in all conditions, and modification of the αRBS sequences did not affect the stability of the mRNA (S4 Fig). We also introduced the αRBS mutations into pfHbp, and found that modifications impaired the thermoregulation of fHbp (S5 Fig), although changing the fHbp sequence affected its detection by western blot analysis. It is likely that the lack of detection of fHbp resulted in changes from the protein sequence (S5 Fig); mutαRBS-1 results in an Ala to Gly substitution, while mutαRBS-2 alters a Cys to Trp, and a Leu to Val (S5 Fig).

Fig 7. αRBS sequences in the open reading frame are necessary for fHbp thermoregulation.

(A) Western blot analysis of fHbp-GFP levels in E. coli harbouring pfHbp-9C-gfp (WT) or the plasmid with modified αRBS-1, αRBS-2 or both (αRBS-1&2). Bacteria were grown at the temperatures indicated to mid-log phase, and cell lysates were subjected to Western blot analysis. The membranes were incubated with antibodies recognising fHbp or RecA. (B) In vitro translation of RNA from E. coli harbouring pfHbp-9C-gfp or plasmids containing altered RBSs (indicated). in vitro translation was performed at the temperatures indicated and subject to Western analysis with antibodies recognising GFP and RecA (loading control). mut-αRBS-1 and mut-αRBS-2 showed reduced thermosensing ability whereas modification of both αRBS-1 and 2 (mut-αRBS-1&2) almost completely abolishes thermoregulation both in E. coli and in in vitro translation assays. Relative values (rel. values) of GFP are indicated below each lane.

Next we examined whether the α-RBS affect the translation of fHbp. in vitro translation reactions were performed with equal amounts of total cellular RNA extracted from E. coli strains harbouring the different constructs, and assays conducted at 30°C, 37°C or 42°C. The in vitro synthesised proteins were extracted and assayed by Western blot analysis. The wild-type construct showed thermoregulation, whereas the three constructs with altered α-RBS did not display thermoregulation (Fig 7B), similar to results found in E. coli; RecA levels were the same for all conditions examined. Taken together, these results demonstrate that both α-RBS sequences contribute to fHbp thermosensing. Additionally, we attempted to introduce the α-RBS mutations into N. meningitidis either under the control of the mono-cistronic or bi-cistronic promoter (S6 Fig). However similar to results in E. coli (S5 Fig), fHbp was undetectable by Western blot analysis of cell lysates of the meningococcus containing mutαRBS-1/2, presumably because the amino acid changes affected the processing of the N-terminal region of fHbp and affected its stability. We considered introducing single C to G mutations into α-RBS1 and/or α-RBS2, but these nucleotide changes of the α-RBSs are not predicted to impact the overall structure of fHbp mRNA (S7 Fig).


The meningococcus has successfully evolved to survive in the human nasopharynx, which is its only natural habitat. Colonisation with this bacterium is frequent in young adults (up to 70% among those living in institutionalised settings such as prisons and barracks) [1], and a single strain can persist in the same individual for months in the upper airway [23]. Within this environment, there are several temperature gradients. For example, the temperature on the surface of the anterior nares is around 30°C at the end of inspiration, and rises to around 34°C in the posterior nasopharynx and tonsillar region [13]. Both these sites on the mucosal surface are significantly cooler than the core body temperature of 37°C, where the bacterium replicates during invasive disease. Additionally, fluctuations in the local temperature will be generated by acute inflammation (resulting in increased blood flow) and systemic illnesses, such as influenza, which provoke a febrile response [24].

We have shown previously that temperature is an important environmental cue for the meningococcus [19]. The production of fHbp and enzymes necessary for capsule biosynthesis and LPS sialylation are increased as the temperature rises from 30°C through to 42°C. The enhancement of immune evasion by the bacterium may reflect transition from the cool anterior portion of the nasopharynx (lined by keratinised squamous cells with little lymphoid tissue) to the warmer posterior nasopharynx, where the meningococcus is found in tonsillar tissue [16]. Furthermore, increased temperature could act as a signal of local inflammation [18] or transition to the sub-mucosal layer, where the bacterium will be exposed to immune effectors.

A notable feature of the meningococcus is its capacity to evade exclusion by the human immune system [4]. Surface structures expressed by N. meningitidis, including Type IV pili, undergo frequent antigenic variation in certain strains [25], while the serogroup B capsule is a molecular mimic of a human post-translational modification [26]. Additionally, fHbp mediates high affinity interactions with the complement regulator, CFH using ligand mimicry [8], and a CFH antagonist CFHR3 [9].

We have shown previously that the biosynthesis of sialic acid-containing capsules is governed by an RNA thermosensor in N. meningitidis [19]. A fundamental advantage of RNA thermosensors is that they operate at the post-transcriptional level [20], so do not require a dedicated sensing pathway or de novo transcription to exert their effect. Therefore, RNA thermosensors are an energetically efficient strategy that offers rapid responses to abrupt changes in the temperature, as seen during the onset of inflammation.

For many bacteria, an increase in temperature is a key signal during their acquisition and ingestion by a mammalian host. For example, in enteric pathogens, RNA thermosensors are known to modulate expression of a transcriptional regulator, which in turn orchestrates the expression of a suite of genes that enable the pathogen to survive in its new environment [20]. Examples include the RNA thermosensors in prfA in Listeria monocytogenes [22], agsA in Salmonella [27], and lcrF in Yersinia spp. [28,29]. Thermosensors also govern iron acquisition systems in Shigella and E. coli [30], and Vibrio cholerae [31]. We found that the prfA thermosensor operates as an ON:OFF switch [32], similar to an RNA thermosensor in Cyanobacteria [33]. The abrupt thermodynamic response of the prfA thermosensor is consistent with Listeria undergoing large temperature fluctuations during its transition from the external environment to the intestinal tract. However, our in vitro transcription/translation assays reveal that the fHbp thermosensor exhibits a gradual change over a range of physiologically relevant temperatures i.e. 32–35°C [17], similar to the N. meningitidis capsule thermosensor [19]. The careful calibration of responses to temperature may be a feature of thermosensors in microbes that exist in close association with thermal gradients within hosts, particularly in the upper airway.

Previous work demonstrated that the expression of fHbp is mediated by bi-cistronic and mono-cistronic transcripts, with the shorter mono-cistronic fHbp transcript controlled by the global regulator of anaerobic metabolism, FNR [21]. Several lines of evidence demonstrate that the mono-cistronic transcript is sufficient but not necessary for fHbp thermoregulation, which is also detected with the bi-cistronic transcript in N. meningitidis. Thermoregulation was detected with the mono-cistronic transcript alone in E. coli and using in vitro transcription/translation assays. Additionally we generated a N. meningitidis mutant lacking the bi-cistronic transcript (by inserting a kanamycin resistance cassette with a terminator upstream of PfHbp). Even though fHbp levels are lower than in the wild-type strain, consistent with previous work [21], the strain still exhibited thermoregulation of fHbp (S6 Fig).

The fHbp transcript is not predicted to contain a ROSE element by RNA structure predictions and does not contain a U(U/C)GCU sequence close to the RBS, which is often present in this class of thermosensors [20]. Furthermore, the potential involvement of a temperature regulated sRNA is unlikely as fHbp thermoregulation occurs both in E. coli and in vitro assays. Instead, our experiments indicate that the mechanism responsible for fHbp thermoregulation depends on two α-RBS sequences located in the fHbp ORF. Modification of each α-RBS independently reduced thermoregulation, which was virtually abolished when both α-RBSs were altered, indicating some redundancy in their function. In contrast, mutation of the fHbp 5´-UTR had little or no effect on thermoregulation. Therefore our results support the model in which the fHbp transcript forms a stem loop at lower temperatures with the RBS occluded by base pairing with one of two α-RBS sequences located in the ORF. Attempts were also made to introduce the α-RBS mutations into N. meningitidis. However, we could not detect fHbp in the meningococcus containing modified α-RBSs (S6 Fig), even though fHbp was detected in E. coli using equivalent constructs on a multi-copy plasmid. The nucleotide changes lead to an alteration in the amino acid sequence of fHbp which might affect lipoprotein localisation and processing, which is distinct in N. meningitidis and E. coli [34]. We considered other modifications to the αRBS sequences. However the wobble rule of RNA:RNA binding [35] means that G can bind several bases (e.g. U and A), so their impact on the secondary structure of the RNA would have been uncertain. The precise contribution of the individual α-RBS sequences to the fHbp RNA thermosensor will be determined in future structural studies.

We also found that the ORF of fHbp contributes to levels of the protein in the meningococcus. Inclusion of first nine codons of fHbp in GFP fusions resulted in significantly higher protein levels of reporter the compared with constructs containing less sequence. This was not mediated by changes in protein stability (S2A Fig), and could result from increased efficiency of translation although these findings need to be confirmed in N. meningitidis.

Of note, attempts were made to generate GFP fusions with 12 and 20 fHbp codons in E. coli to define sequences required for maximal fHbp expression. However, it was not possible to obtain the fHbp12C-gfp and fHbp20C-gfp constructs. fHbp is a surface lipoprotein bound to the outer membrane via an N-terminal lipid anchor [10,11]. Unlike in the meningococcus, we have been unable to detect fHbp on the surface of E. coli even when expressing the full length protein, demonstrating that there are differences in protein sorting in these two Gram negative bacteria. It is therefore possible that additional fHbp sequences in gfp fusions cause accumulation of GFP at aberrant cellular sites, impairing bacterial viability.

fHbp thermoregulation may have implications for the effect of vaccines that target fHbp. Levels of this vaccine antigen in the meningococcus in the upper airway (at 32–35°C) may be lower than in assays to assess immune responses within the laboratory, which are typically performed at 37°C [36,37]. Therefore, vaccines that include fHbp might not impose selective pressure on bacteria at the mucosal surface in the upper airway, and offer limited herd immunity [38]. This is consistent with a recent study demonstrating that immunisation with a vaccine containing fHbp has a limited impact on the acquisition of meningococcal carriage among university students [39].

Aside from factors involved in immune evasion, RNA thermometers may control other features in N. meningitidis and other bacteria that inhabit the nasopharynx. Previous studies have focused mainly on the effect of temperature on mRNA levels in the meningococcus [40]. The identification of further RNA thermosensors will require bio-informatic and proteomic approaches. Further understanding the mechanisms of thermoregulation could be informative about strategies of immune evasion employed by this important pathogen, its adhesive properties, and the acquisition of relevant nutrients at different sites in the upper airways [41].


Strains, plasmids and culture conditions

N. meningitidis was grown in Brain Heart Infusion broth (BHI, Oxoid, 37 g dissolved in 1 L dH2O with 1 g starch) or on BHI agar (1.5% w/v) supplemented with 5% Levinthal’s base (500 ml defibrinated horse blood, autoclaved with 1 L BHI broth). Bacteria on solid media were incubated for 16–18 hours at 37˚C with 5% CO2. Liquid cultures (10 ml) were inoculated with 109 bacteria and grown at 37˚C with shaking (180 r.p.m.) to an optical density (O.D.) measured at 600 nm of ~0.5 unless otherwise stated.

E. coli was grown in Luria-Bertani (LB) broth (2% w/v in dH2O, Oxoid, UK) or on LB agar (1% w/v) plates. Liquid cultures of E. coli were grown in 4 ml of media inoculated from a single colony overnight at 37˚C with shaking (180 r.p.m.). Overnight grown bacteria were diluted 1 in 100 in media and grown to an Optical Density (OD) A600 of ~0.5. When necessary antibiotics were added to the following final concentrations: carbenicillin, 100 μg ml-1; kanamycin, 50 μg ml-1; rifampicin, 250 μg ml-1. The strains and plasmids used in this study are listed in Table 1.

Flow cytometry

N. meningitidis was grown in liquid culture to mid. log phase at 30°C, 37°C or 42°C, prior to fixation for two hours in 3% paraformaldehyde. Surface localisation of fHbp on N. meningitidis was detected using anti-fHbp V1.1 pAbs and goat anti-mouse IgG-Alexa Fluor 647 conjugate (Molecular Probes, LifeTechnologies). Samples were run on a FACSCalibur (BD Biosciences), and at least 104 events recorded before results were analysed by calculating the geometric mean fluorescence intensity in FlowJo vX software (Tree Star).

Plasmids and construction of N. meningitidis mutants

A N. meningitidis strain containing only the monocistronic fHbp transcript was generated by insertion of a kanamycin resistance cassette with a Rho-independent terminator upstream of PfHbp (S6 Fig). Upstream and downstream fragments, and the kanamycin resistance cassette were amplified by from gDNA using the primer pairs fHbp-KM-(1)-F/fHbp-KM-(1)-R, fHbp-KM-(2)-F/fHbp-KM-(2)-R and fHbp-KM-(3)-F/fHbp-KM-(3)-R, respectively. Details of primers used in this study are given in Table 2. PCR products were ligated into pGEM-T (Promega) following Gibson Assembly (NEB), then digested with NcoI and NotI (NEB). Transformation of N. meningitidis strain MC58 was performed as described previously [42].

N. meningitidis MC58 containing only the bicistronic fHbp transcript was generated by replacing the nmb1869 (the gene upstream of fHbp) with the kanamycin resistance gene only, leaving the nmb1869 promoter intact while PfHbp was disrupted by changing the -10 sequence (TACCATAA to TACCATCC). Upstream and downstream fragments, and the kanamycin resistance cassette together with the modified -10 region mutation were amplified using the primer pairs prom-10-mut1-F/prom-10-mut1-R, prom-10-mut3-F/prom-10-mut3-R, prom-10-mut4-F/prom-10-mut4-R, prom-10-mut5-F/prom-10-mut5-R with genomic DNA as the target, while primers prom-10-mut2-F/prom-10-mut2-R, were used to amplify the kanamycin resistance cassette. PCR products were ligated into pGEM-T (Promega) following Gibson Assembly (NEB), and then digested with NcoI and NotI before being used to transform N. meningitidis.

Site-directed mutagenesis was performed with the Quickchange kit (Stratagene) according to the manufacturer’s protocol. To modify fHbp9C-GFP (introducing mut1, mut2, mut3, mut4, mut-αRBS-1, mut-αRBS-2 and mut-αRBS-1&2), oligonucleotides pairs mut1-F/mut1-R, mut2-F/mut2-R, mut3-F/mut3-R, mut4-F/mut4-R, mut-αRBS-1-F/mut-αRBS-1-R, mut-αRBS-2-F/Mut-αRBS-2-R, mut-αRBS-1&2-F/mut-αRBS-1&2-R were used respectively (Table 2). The reaction products were transformed into E. coli DH5α, and constructs were confirmed by sequencing.

Full length fHbp was amplified from N. meningitidis MC58 using primers fHbp(c)-F and fHbp(c)-R and ligated into pGEMT to yield pfHbp. Deletions were generated by PCR and the products were then ligated into pGEM-T (Promega) and transformed into E. coli DH5α. The identity of all constructs was confirmed by nucleotide sequencing.

Plasmids containing GFP fusions were generated by amplifying the promoter of fHbp with different lengths of the ORF with fHbp(TTS)-U or fHbp-GFP-F with either fHbp-GFP1C-R, fHbp-GFP5C-R or fHbp-GFP9C-R, and ligating the products into pEGFP-N2 (Clontech).

RNA isolation and northern blot analysis

N. meningitidis was grown in liquid culture to mid. log phase, and RNA was isolated using the RNAeasy Miniprep Kit (Qiagen, UK) following the manufacturer’s protocol. For E. coli, bacteria were grown in liquid media to mid log phase, and RNA isolated using the FastRNA Pro Blue kit (MP Biomedicals) according to the manufacturer’s protocol. The purity and integrity of RNA were determined by gel electrophoresis and spectrophotometry.

For Northern blotting, 20 μg of total RNA was separated on a formaldehyde agarose gel prior to blotting as described previously [43], then transferred to Hybond N. Membranes were hybridised with 32P-ATP ɣ-labelled DNA fragments Northern blots were developed using a Fuji phosphorImager scanner. Probes for detecting fHbp and tmRNA were amplified from gDNA with primer pairs fHbp-U/fHbp-D, and tmRNA-U/tmRNA-D, respectively.

To analyse mRNA stability, E. coli containing relevant plasmids was grown in liquid culture to an OD600nm of 0.5–0.6 then exposed to rifampicin (250 μg ml-1 final concentration) and incubated at 37°C with agitation. Bacteria were harvested for RNA isolation 0, 5, 10 and 20 minutes afterwards. Blots were probed with a labelled oligonucleotides GGTGCAGATGAACTTCAGGGTCAGCTTGCCGTAGGTGGCATCGCCCTCGC (to detect GFP mRNA), and a tmRNA product amplified from E. coli gDNA with primers Tm1 and Tm2 (Table 2). Band intensities of Northern blots were quantified using AIDA image analyzer software, standardised to the tmRNA loading control, and expressed as a ratio to the respective band intensities at t = 0 min.

SDS-PAGE, western blotting and protein stability

Cell lysates were prepared by addition of SDS:PAGE loading buffer to an equal volume of bacteria obtained from liquid cultures by centrifugation. Total protein levels were measured using a Bradford assay and equal amounts of total protein loaded into each lane. Samples were boiled, then the proteins separated on polyacrylamide gels and transferred to immobolin P polyvinylidine fluoride (PVDF) membranes (Millipore, USA) using semi-dry transfer (Biorad, USA). For Western blot analysis, membranes were washed three times in 0.05% (w/v) dry milk/PBS with 0.05% (v/v) Tween-20 for 10 minutes, and then incubated with the primary antibody for one hour. Membranes were washed again three times and incubated for a further hour with a secondary, HRP-conjugated antibody. Binding was detected with an ECL Western Blotting Detection kit (Amersham, USA) and exposed to ECL Hyperfilm. An α-GFP mouse antibody (BD-living colors) was used at a final dilution of 1:8,000. α-fHbp polyclonal sera was used at a final dilution of 1:5000. α-RecA rabbit antibody (Abcam, UK) was used at a final dilution of 1:10,000. As secondary antibodies, goat α-rabbit or α -mouse IgG HRP-conjugated antibody (Dako, UK) was used at a final dilution of 1:10,000.

To determine protein stability, translation was prevented by adding spectinomycin (Sigma, final concentration 100 μg ml-1) to bacteria grown to an OD600  =  0.5 in liquid media. Samples were removed at times afterwards for Western blot analysis. Relative expression was calculated by measuring band intensities with ImageJ software, standardised to signals for loading controls (i.e. RecA or tmRNA), and shown as the ratio, relative to intensity of the control strain or condition.

In vitro transcription/translation and prediction of RNA folding

For the template, DNA was isolated from derivatives of pEGFP-N2 containing one, five or nine codons of fHbp fused to GFP (GenElute Gel Extraction Kit, Sigma), linearised by digestion with NotI (New England Biolabs) and then purified using QIAquick (Qiagen). For RNA and DNA templates, 1 μg of nucleic acid was used as a template. The in vitro transcription/translation reaction was performed at 30°C, 37°C or 42°C for one hour using the E. coli S30 Extract system for Linear Templates in vitro Transcription/Translation Kit (Promega). The products were precipitated in acetone, then re-suspended in SDS-PAGE buffer prior to Western blot analysis.

RNA sequences were analysed using the RNAfold web server of the Vienna RNA package ( For each sequence, the minimum free energy in kcal mol−1 was predicted [44].

Supporting Information

S1 Fig. Thermoregulation of fHbp in E. coli occurs irrespective of the orientation in a plasmid.

E. coli containing a plasmid with fHbp lacking the FNR box and Pfhbp but under the control of the SP6 promoter was grown at the temperatures indicated until mid-log, then protein was obtained from whole cell lysates and examined by Western blot using antibodies against fHbp and RecA (as a loading control).


S2 Fig. Stability of the GFP reporter and mRNA in E. coli.

(A) Bacteria containing pfHbp-1c-gfp or pfHbp-9c-gfp was grown at 37°C to mid log phase, before protein synthesis was blocked by addition of spectinomycin. Samples were removed at indicated time-points and subjected Western blot analysis. Membranes were probed with antibodies recognising GFP or RecA (loading control). (B) Bacteria were harvested for RNA isolation after 5, 10 and 20 minutes of incubation at 37°C with agitation after the addition of rifampicin (250 μg/ml) to inhibit RNA synthesis. Total RNA (15 μg) from each sample were separated agarose formaldehyde gels and analysed by Northern blotting using probes for gfp and tmRNA. (C) Band intensities of the gfp transcripts were quantified using AIDA image analyzer software, standardised to the tmRNA loading control, and expressed as a ratio to the respective band intensities at t = 0 min.


S3 Fig. Putative RNA secondary structures of the fHbp-nc-gfp constructs.

Colours of nucleotides show base-pair probabilities as calculated by the Vienna RNAfold programme (RBS indicated in blue and start codon in red).


S4 Fig. Modification of αRBS sequences does not affect mRNA stability.

(A) After growth to mid-log phase, bacteria were harvested for RNA isolation after 5, 10 and 20 minutes of incubation at 37°C with agitation after the addition of rifampicin (250 μg/ml) to inhibit RNA synthesis. Total RNA (15 μg) from each sample were separated agarose formaldehyde gels and analysed by Northern blotting using probes for gfp and tmRNA. (B) Band intensities of the gfp transcripts were quantified using AIDA image analyzer software, standardised to the tmRNA loading control, and expressed as a ratio to the respective band intensities at t = 0 min.


S5 Fig. Modification of the a-RBSs in pfHbp influences thermosensing.

(A) Mutagenesis of the mut-αRBSs in fHbp. Altered nucleotides are indicated in red, while the boxes show the predicted amino acid sequence. +1 indicates first nucleotide of the fHbp start codon. (B) Western blot analysis examining fHbp levels in E. coli containing modified pfHbp. Bacteria were grown at various temperatures overnight on solid media and protein isolated from whole cell lysates. Membranes were probed with antibodies recognising fHbp or RecA (loading control). (C) Quantification of fHbp levels performed by ImageJ analysis of Western blots probed with a-fHbp or a-RecA pAbs. Results normalised to the relative fHbp:RecA value obtained for pfHbp with mutαRBS-1 grown at 30°C as 100%. Experiments were performed on three indepdent occasions and error bars show the S.D.


S6 Fig. Modification of the a-RBSs in N. meningitidis.

(A) Schematic diagram of the fhbp operon with the site of the insertion of the kanamycin resistance cassette. fhbp expression in N. meningitidis is regulated by two independent promoters (shown in arrows), yielding a 1,946 nt. bi-cistronic transcript and a 825 nt. mono-cistronic message generated from the promoter, PfHbp. The FNR box is in orange. Green dotted lines denote insertion site of an kanamycin cassette with its own terminator to disrupt the bi-cistronic transcript. (B, C) Western blot analysis examining fHbp levels in N. meningitidis Bacteria were grown at various temperatures overnight on solid media and protein isolated from whole cell lysates. Membranes were probed with antibodies recognising fHbp or RecA (loading control). Strains with fHbp under the control of the mono-cistronic (B) or bi-cistronic (C) fHbp promoters were examined. Construction of the strain lacking the monocistronic fHbp promoter is described in Fig 3A.


S7 Fig. Predicted secondary RNA structures for modified fHbp mRNAs.

Colours of nucleotides show base-pair probabilities as calculated by the Vienna RNAfold programme, with the predicted minimum free energies in kcal/mole for fHbp mRNAs with a single C to G change in (A) αRBS1, (B) αRBS1, and (C) αRBS1 and αRBS2. The positions of the modified bases are shown.


Author Contributions

  1. Conceived and designed the experiments: EL HL FT AT CMT.
  2. Performed the experiments: EL HL FT AT.
  3. Analyzed the data: EL HL FT AT CMT.
  4. Wrote the paper: EL HL FT CMT.


  1. 1. Yazdankhah SP, Caugant DA (2004) Neisseria meningitidis: an overview of the carriage state. J Med Microbiol 53: 821–832. pmid:15314188
  2. 2. Stephens DS, Greenwood B, Brandtzaeg P (2007) Epidemic meningitis, meningococcaemia, and Neisseria meningitidis. Lancet 369: 2196–2210. pmid:17604802
  3. 3. Rosenstein NE, Perkins BA, Stephens DS, Popovic T, Hughes JM (2001) Meningococcal disease. N Engl J Med 344: 1378–1388. pmid:11333996
  4. 4. Lo H, Tang CM, Exley RM (2009) Mechanisms of avoidance of host immunity by Neisseria meningitidis and its effect on vaccine development. The Lancet infectious diseases 9: 418–427. pmid:19555901
  5. 5. Densen P (1989) Interaction of complement with Neisseria meningitidis and Neisseria gonorrhoeae. Clin Microbiol Rev 2 Suppl: S11–17. pmid:2497954
  6. 6. Davila S, Wright VJ, Khor CC, Sim KS, Binder A, et al. (2010) Genome-wide association study identifies variants in the CFH region associated with host susceptibility to meningococcal disease. Nature genetics 42: 772–776. pmid:20694013
  7. 7. Schneider MC, Exley RM, Chan H, Feavers I, Kang YH, et al. (2006) Functional significance of factor H binding to Neisseria meningitidis. Journal of immunology 176: 7566–7575.
  8. 8. Schneider MC, Prosser BE, Caesar JJ, Kugelberg E, Li S, et al. (2009) Neisseria meningitidis recruits factor H using protein mimicry of host carbohydrates. Nature 458: 890–893. pmid:19225461
  9. 9. Caesar JJ, Lavender H, Ward PN, Exley RM, Eaton J, et al. (2014) Competition between antagonistic complement factors for a single protein on N. meningitidis rules disease susceptibility. eLife 3.
  10. 10. Masignani V, Comanducci M, Giuliani MM, Bambini S, Adu-Bobie J, et al. (2003) Vaccination against Neisseria meningitidis using three variants of the lipoprotein GNA1870. The Journal of experimental medicine 197: 789–799. pmid:12642606
  11. 11. Fletcher LD, Bernfield L, Barniak V, Farley JE, Howell A, et al. (2004) Vaccine potential of the Neisseria meningitidis 2086 lipoprotein. Infection and immunity 72: 2088–2100. pmid:15039331
  12. 12. McFadden ER Jr., Pichurko BM, Bowman HF, Ingenito E, Burns S, et al. (1985) Thermal mapping of the airways in humans. Journal of applied physiology 58: 564–570. pmid:3980358
  13. 13. Keck T, Leiacker R, Riechelmann H, Rettinger G (2000) Temperature profile in the nasal cavity. Laryngoscope 110: 651–654. pmid:10764013
  14. 14. Cole P (1953) Some aspects of temperature, moisture and heat relationships in the upper respiratory tract. The Journal of laryngology and otology 67: 449–456. pmid:13085046
  15. 15. McFadden ER Jr., Pichurko BM (1985) Intraairway thermal profiles during exercise and hyperventilation in normal man. The Journal of clinical investigation 76: 1007–1010. pmid:4044825
  16. 16. Sim RJ, Harrison MM, Moxon ER, Tang CM (2000) Underestimation of meningococci in tonsillar tissue by nasopharyngeal swabbing. Lancet 356: 1653–1654. pmid:11089827
  17. 17. Keck T, Leiacker R, Heinrich A, Kuhnemann S, Rettinger G (2000) Humidity and temperature profile in the nasal cavity. Rhinology 38: 167–171. pmid:11190750
  18. 18. Cabanac M, editor (1990) Phylogeny of fever. Berlin: Springer Verlag. 284–296 p.
  19. 19. Loh E, Kugelberg E, Tracy A, Zhang Q, Gollan B, et al. (2013) Temperature triggers immune evasion by Neisseria meningitidis. Nature 502: 237–+. pmid:24067614
  20. 20. Kortmann J, Narberhaus F (2012) Bacterial RNA thermometers: molecular zippers and switches. Nature reviews Microbiology 10: 255–265. pmid:22421878
  21. 21. Oriente F, Scarlato V, Delany I (2010) Expression of factor H binding protein of meningococcus responds to oxygen limitation through a dedicated FNR-regulated promoter. Journal of bacteriology 192: 691–701. pmid:19948796
  22. 22. Johansson J, Mandin P, Renzoni A, Chiaruttini C, Springer M, et al. (2002) An RNA thermosensor controls expression of virulence genes in Listeria monocytogenes. Cell 110: 551–561. pmid:12230973
  23. 23. Ala'Aldeen DA, Neal KR, Ait-Tahar K, Nguyen-Van-Tam JS, English A, et al. (2000) Dynamics of meningococcal long-term carriage among university students and their implications for mass vaccination. Journal of clinical microbiology 38: 2311–2316. pmid:10834994
  24. 24. Eccles R (2005) Understanding the symptoms of the common cold and influenza. The Lancet Infectious diseases 5: 718–725. pmid:16253889
  25. 25. Wormann ME, Horien CL, Bennett JS, Jolley KA, Maiden MC, et al. (2014) Sequence, distribution and chromosomal context of class I and class II pilin genes of Neisseria meningitidis identified in whole genome sequences. BMC genomics 15: 253. pmid:24690385
  26. 26. Finne J, Leinonen M, Makela PH (1983) Antigenic similarities between brain components and bacteria causing meningitis. Implications for vaccine development and pathogenesis. Lancet 2: 355–357. pmid:6135869
  27. 27. Waldminghaus T, Heidrich N, Brantl S, Narberhaus F (2007) FourU: a novel type of RNA thermometer in Salmonella. Molecular microbiology 65: 413–424. pmid:17630972
  28. 28. Hoe NP, Minion FC, Goguen JD (1992) Temperature sensing in Yersinia pestis: regulation of yopE transcription by lcrF. Journal of bacteriology 174: 4275–4286. pmid:1624422
  29. 29. Bohme K, Steinmann R, Kortmann J, Seekircher S, Heroven AK, et al. (2012) Concerted actions of a thermo-labile regulator and a unique intergenic RNA thermosensor control Yersinia virulence. PLoS pathogens 8: e1002518. pmid:22359501
  30. 30. Kouse AB, Righetti F, Kortmann J, Narberhaus F, Murphy ER (2013) RNA-mediated thermoregulation of iron-acquisition genes in Shigella dysenteriae and pathogenic Escherichia coli. PloS one 8: e63781. pmid:23704938
  31. 31. Weber GG, Kortmann J, Narberhaus F, Klose KE (2014) RNA thermometer controls temperature-dependent virulence factor expression in Vibrio cholerae. Proceedings of the National Academy of Sciences of the United States of America 111: 14241–14246. pmid:25228776
  32. 32. Loh E, Kugelberg E, Tracy A, Zhang Q, Gollan B, et al. (2013) Temperature triggers immune evasion by Neisseria meningitidis. Nature 502: 237–240. pmid:24067614
  33. 33. Cimdins A, Klinkert B, Aschke-Sonnenborn U, Kaiser FM, Kortmann J, et al. (2014) Translational control of small heat shock genes in mesophilic and thermophilic cyanobacteria by RNA thermometers. RNA biology 11: 594–608. pmid:24755616
  34. 34. Hooda Y, Lai CC-L, Judd A, Buckwalter CM, Shin HE, et al. (2016) Slam is an outer membrane protein that is required for the surface display of lipidated virulence factors in Neisseria. Nature Microbiology 1: 16009.
  35. 35. Murphy FVt, Ramakrishnan V (2004) Structure of a purine-purine wobble base pair in the decoding center of the ribosome. Nature structural & molecular biology 11: 1251–1252.
  36. 36. Pizza M, Scarlato V, Masignani V, Giuliani MM, Arico B, et al. (2000) Identification of vaccine candidates against serogroup B meningococcus by whole-genome sequencing [see comments]. Science 287: 1816–1820. pmid:10710308
  37. 37. Johnson S, Tan L, van der Veen S, Caesar J, Goicoechea De Jorge E, et al. (2012) Design and evaluation of meningococcal vaccines through structure-based modification of host and pathogen molecules. PLoS pathogens 8: e1002981. pmid:23133374
  38. 38. Trotter CL, Maiden MC (2009) Meningococcal vaccines and herd immunity: lessons learned from serogroup C conjugate vaccination programs. Expert review of vaccines 8: 851–861. pmid:19538112
  39. 39. Read RC, Baxter D, Chadwick DR, Faust SN, Finn A, et al. (2014) Effect of a quadrivalent meningococcal ACWY glycoconjugate or a serogroup B meningococcal vaccine on meningococcal carriage: an observer-blind, phase 3 randomised clinical trial. Lancet 384: 2123–2131. pmid:25145775
  40. 40. Guckenberger M, Kurz S, Aepinus C, Theiss S, Haller S, et al. (2002) Analysis of the heat shock response of Neisseria meningitidis with cDNA- and oligonucleotide-based DNA microarrays. Journal of bacteriology 184: 2546–2551. pmid:11948171
  41. 41. Exley RM, Shaw J, Mowe E, Sun YH, West NP, et al. (2005) Available carbon source influences the resistance of Neisseria meningitidis against complement. J Exp Med 201: 1637–1645. pmid:15897277
  42. 42. Exley RM, Goodwin L, Mowe E, Shaw J, Smith H, et al. (2005) Neisseria meningitidis lactate permease is required for nasopharyngeal colonization. Infection and immunity 73: 5762–5766. pmid:16113293
  43. 43. Toledo-Arana A, Dussurget O, Nikitas G, Sesto N, Guet-Revillet H, et al. (2009) The Listeria transcriptional landscape from saprophytism to virulence. Nature 459: 950–956. pmid:19448609
  44. 44. Hofacker IL (2003) Vienna RNA secondary structure server. Nucleic Acids Res 31: 3429–3431. pmid:12824340