Abstract
Type III secretion systems (T3SSs) are utilized by numerous Gram-negative bacteria to efficiently interact with host cells and manipulate their function. Appropriate expression of type III secretion genes is achieved through the integration of multiple control elements and regulatory pathways that ultimately coordinate the activity of a central transcriptional activator usually belonging to the AraC/XylS family. Although several regulatory elements are conserved between different species and families, each pathogen uses a unique set of control factors and mechanisms to adjust and optimize T3SS gene expression to the need and lifestyle of the pathogen. This is reflected by the complex set of sensory systems and diverse transcriptional, post-transcriptional and post-translational control strategies modulating T3SS expression in response to environmental and intrinsic cues. Whereas some pathways regulate solely the T3SS, others coordinately control expression of one or multiple T3SSs together with other virulence factors and fitness traits on a global scale. Over the past years, several common regulatory themes emerged, e.g., environmental control by two-component systems and carbon metabolism regulators or coupling of T3SS induction with host cell contact/translocon-effector secretion. One of the remaining challenges is to resolve the understudied post-transcriptional regulation of T3SS and the dynamics of the control process.
Marcel Volk and Ines Vollmer contributed equally
Access provided by Autonomous University of Puebla. Download chapter PDF
Similar content being viewed by others
1 Introduction
Type III secretion systems (T3SS) are complex nanomachines of Gram-negative bacterial pathogens of plants, animals and humans that export proteins (called effectors) from the bacterial cytoplasm across the cell envelope and inject them into host cells during infection (Büttner 2012; Portaliou et al. 2016; Galan et al. 2014; Deng et al. 2017; Hueck 1998). Depending on the individual pathogen, the injected effectors act as toxins, adhesins or enzymes and can promote attachment and invasion into host cells, intracellular survival and replication or prevent host defenses. The T3SS is composed of 30–40 proteins that are assembled into a needle-like injectisome structure where they are incorporated as single molecules or in few or multiple copies (Galan et al. 2014; Deng et al. 2017; Diepold and Wagner 2014). Consequently, the synthesis of the T3SS proteins that form or utilize the machinery follows a strict hierarchy (Galan et al. 2014; Diepold and Wagner 2014). Moreover, synthesis, recruitment and unfolding as well as secretion and delivery of the effector proteins into host cells are highly energy consuming processes. This is particular evident by the fact that several pathogens stop growth and replication when the T3SS is induced (Büttner 2012; Portaliou et al. 2016; Deng et al. 2017). Thus, it is not surprising that the production of the T3SS in pathogens is tightly controlled by a plethora of regulatory factors in response to numerous environmental cues and the secretory activity of the injectisome. They act on the transcriptional, post-transcriptional and post-translational level and form a complex feedback-controlled network. In the following overview, we focus on the wealth of T3SS control factors of important human pathogens and discuss current challenges to examine their functions.
2 T3SS Regulation on the Transcriptional Level
2.1 Control by Central Transcriptional Activators
The first central factors identified to regulate the expression of the T3SS components were dimeric, transcriptional activators of the AraC/XylS family. This family of activators includes LcrF/VirF in human pathogenic yersiniae, HilD, HilC and RtsA in Salmonella enterica, MxiE in Shigella flexneri and ExsA in Pseudomonas aeruginosa (Francis et al. 2002). A common regulatory principle of these key activators involves the coordinate control of all or of a large subset of components and substrates of the T3SS in the respective pathogen. In several cases, multiple binding sites have been identified upstream the target genes and operons (Schwiesow et al. 2015).
In general, all transcriptional activators of this class are composed of an N-terminal sensing domain for environmental signals and a C-terminal helix-turn-helix (HTH) DNA-binding domain per subunit. DNA binding occurs through the recognition helix in the HTH that binds to specific DNA residues within the major groove (Bustos and Schleif 1993; Schleif 2010). Interestingly, some of these master activators, such as LcrF/VirF of Yersinia and ExsA of P. aeruginosa, are highly homologous and can complement each other. They were shown to interact with common nucleotide sequence motifs that are often highly variable regarding the distance to the transcriptional start sites, directionality and sequence conservation (Schwiesow et al. 2015; King et al. 2013). Notably, despite the resemblance of the DNA motifs, the oligomeric state of the LcrF/VirF (dimer) and ExsA (monomer) proteins is different when they are recruited to the binding sites. This ultimately results in distinct binding affinities, promoter bending and different kinetics of transcriptional activation (Schwiesow et al. 2015; King et al. 2013). Some of the N-terminal domains were further shown to bind co-factors that induce conformational changes and influence the ability of the protein to regulate transcription. One recent study for example showed that the crucial regulator HilD of S. enterica binds long-chain fatty acids such as oleate, which prevents binding of the activator to its target sites (Golubeva et al. 2016) (for more details, see Sect. 4.2).
Additionally, many important bacterial pathogens, including S. enterica, possess multiple T3SSs in which the key regulators of the systems are also implicated in the control of the master regulator of the other T3SSs. For instance, HilD coordinates the expression of two other type III secretion machineries of Salmonella, the flagellar T3SS and the Salmonella pathogenicity island 2 (SPI-2) encoded injectisome required for host defenses (Ellermeier and Slauch 2007) (Fig. 1).
2.2 Transcriptional Control of the Key T3SS Regulators
Appropriate expression of T3SS components is generally achieved through the integration of several regulatory factors and pathways in the form of a highly structured network that ultimately control the activity of the central AraC/XylS-type transcription activator. This enables the bacteria to tightly control and adjust the production of the T3SS in response to unique environmental cues encountered in the respective host niches. In S. enterica, control of the T3SS-1 (encoded on the Salmonella pathogenicity island 1 (SPI-1)) is mediated by the AraC/XylS proteins HilC, HilD and RtsA (Erhardt and Dersch 2015) (Fig. 1). They regulate each other and the transcription of their own gene and independently activate the promoter of the OmpR/ToxR family activator HilA. HilA primarily induces transcription of the structural components of the SPI-1 gene cluster, including prg/org and inv/spa (Ellermeier et al. 2005). Most environmental signals that regulate SPI-1 gene expression are sensed by two-component systems and integrated on the level of HilD. The response to (i) osmolarity, desiccation and low temperature occurs through the two-component systems OmpR/EnvZ and the RcsCD/RcsB, and (ii) presence of certain metabolites is sensed through the BarA/SirA two-component system (Erhardt and Dersch 2015). Hence, HilD constitutes the key activator of Salmonella T3SS genes, whereas HilC and RtsA rather act as amplifiers of the activating signal. Control of the key regulator LcrF/VirF of the Yersinia T3SS, which is encoded on the Yersinia virulence plasmid (pYV), is similarly complex (Fig. 2). Its expression is tightly controlled by nutrients, Mg2+ and pH, through the BarA/SirA, PhoP/PhoQ-CsrABC cascade and the cyclic AMP receptor protein (Crp). In addition, diverse cell stresses can be sensed through the two-component systems RcsCD/RcsB and CpxA/CpxR (Schwiesow et al. 2015).
Expression of the T3SS master activators is often further influenced by the action of specific transcriptional regulators that promote activator transcription only under certain environmental conditions. Examples of important environmental parameters in this context are the availability of oxygen and ferric/ferrous ions. In this context, Ellermeier and Slauch and Teixido et al. (Ellermeier and Slauch 2008; Teixido et al. 2011) found that the ferric uptake regulator Fur controls HilD expression and more recent studies identified the iron–sulfur cluster coordinating transcriptional regulator IscR as an important transcriptional repressor of the LcrF/VirF and HilD master regulators of Yersinia and Salmonella (Miller et al. 2014; Vergnes et al. 2017) (Figs. 1 and 2). It is assumed that iron limitation, oxidative stress, as well as oxygen limitation as a result of Fe–S cluster damage, affect the activity of IscR. Another common global regulatory protein is the LysR homologue LrhA. While this regulator represses flagella T3SS expression in Escherichia coli and Salmonella, it, on the contrary, induces the espA gene of the pathogenicity island locus of enterocyte effacement (LEE) of enterohemorrhagic E. coli (EHEC) and the rtsB regulator gene of SPI-1 genes in Salmonella (Erhardt and Dersch 2015; Shimizu et al. 2015).
Another common feature is that expression of the master T3SS regulators is also governed by global regulators. They are needed for metabolic adaptation and can additionally coordinate expression of the T3SSs with available carbon sources. Among these regulators is Crp. Crp primarily helps the pathogens to manage and optimize their metabolism by checking and ranking uptake and utilization of available and readily digestible carbon sources (Görke and Stülke 2008; Poncet et al. 2009). In this context, Crp is also important to link the nutrient status and carbon metabolism with the regulation of the T3SS either directly or via the control of the post-transcriptional carbon storage regulator system (Csr), which affects the expression of multiple master regulators in many pathogens (for details see Sect. 3.1.2) (Kusmierek and Dersch 2017; Vakulskas et al. 2015).
2.3 Silencing and Activation of T3SS Master Regulator Expression by Modulator Proteins
Under non-inducing conditions, e.g., outside the host, T3SS genes are often subjected to silencing by ancestral nucleoid-structuring proteins of the H-NS and the Hha/YmoA family. These global modulators of gene expression are implicated in the xenogeneic repression of many virulence genes with a low GC-content that were acquired by horizontal gene transfer (Navarre et al. 2006; Dorman 2007). H-NS and HhA/YmoA preferentially bind to AT-rich bent promoter regions, and their binding sites often overlap with binding sites of positive transcriptional activators that are able to alleviate transcriptional repression. This silencing and anti-silencing mechanism was found for H-NS and Hha for all three AraC/XylS-type transcriptional activators RtsA, HilC and HilD which control T3SS genes in S. enterica (Olekhnovich and Kadner 2007) (Fig. 1). Similarly, Ler (LEE-encoded regulator), a master regulator of the LEE operons of enteropathogenic E. coli (EPEC) and EHEC, is able to relieve H-NS mediated silencing of the LEE5 promoter (Laaberki et al. 2006) (Fig. 3). The LEE-encoded T3SS promotes the establishment of intimate attachment structures (intimin-mediated pedestals) of EPEC/EHEC via translocated effectors leading to attaching and effacing (A/E) lesions and severe damage of the intestinal villi (Katsowich et al. 2017; Bhatt et al. 2009). This is enabled by the significantly higher binding affinity (about 40-fold) of the T3SS master activator Ler to the LEE target DNA sequences, in comparison to H-NS (Choi et al. 2016).
Interestingly, members of the H-NS and Hha/YmoA family are also able to form heterodimers. How this interaction modulates expression of their target genes is not clear yet, as the influence of both family members on gene expression varies significantly between the different pathogens. However, some evidence exists that heterodimer formation influences the binding affinity to their target sites and links control of the affected genes to other environmental control systems (Madrid et al. 2002, 2007). One striking example is the formation of H-NS and YmoA complexes in human pathogenic yersiniae. YmoA is important to block transcription of the T3SS master regulator gene lcrF/virF in Yersinia to silence sequences downstream of the lcrF/virF promoter (Böhme et al. 2012) (Fig. 2). In contrast to its E. coli homologue, it is preferentially degraded by the Lon and Clp proteases at body temperature, leading to derepression of lcrF/virF transcription upon infection (Jackson et al. 2004).
3 T3SS Regulation on the Post-transcriptional Level
3.1 Control of Translation
3.1.1 Sensory RNAs—RNA Thermometers
One of the first post-transcriptional control mechanisms of T3SS gene expression was discovered in Yersinia. A comparison of the amount of the T3SS master regulator at different growth temperatures revealed that the efficiency of lcrF/virF mRNA translation was strongly increased at mammalian body temperature (i.e., 37 °C) (Hoe and Goguen 1993). Initial mRNA secondary structure predictions suggested that the lcrF ribosome binding site (RBS) is incorporated into a stem-loop. In a later study, the 5′-untranslated region (5′-UTR) of the lcrF/virF mRNA was mapped, and structure probing identified a unique cis-acting RNA element which forms a two stem-loop structure at moderate temperatures. The first stem-loop stabilizes the second stem-loop which sequesters the lcrF/virF RBS by a stretch of four uracils. Opening of this structure is favored at 37 °C and permits ribosome binding at host body temperature (Böhme et al. 2012; Rhigetti et al. 2016) (Fig. 2). The biological relevance of this RNA thermometer was verified in animal models with two different Yersinia pseudotuberculosis strains expressing a stabilized and a labile variant of the RNA thermometer. The stabilized variant was strongly reduced in its ability to disseminate into the Peyer’s patches, liver and spleen and had fully lost its lethality due to the lack of lcrF expression, whereas the destabilized version of the thermosensor was attenuated or exhibited a similar, but not a higher mortality (Böhme et al. 2012). This illustrated that the evolved RNA thermometer provides just the appropriate amount of the T3SS master regulator at the appropriate condition and time for an optimal infection efficiency of Yersinia.
3.1.2 Translational Control by CsrA/RsmA RNA-Binding Proteins
CsrA/RsmA-type RNA-binding proteins belong to a multicomponent, post-transcriptional regulatory control system that adjusts expression of T3SS genes in several Gram-negative pathogens. A key function of CsrA/RsmA protein family members is the coordinate adaptation of virulence traits, metabolic functions and physiological properties to optimize virulence and fitness of the pathogen during the different stages of the infection (Kusmierek and Dersch 2017; Vakulskas et al. 2015). CsrA/RsmA proteins most commonly prevent the translation of their numerous target mRNAs, including multiple T3SS gene transcripts. They usually bind to GGA-containing sequences that are exposed in single-stranded loop regions of two or more stem-loop structures residing in the 5’-UTRs of the impacted mRNAs, of which one includes the RBS. Simultaneous interaction of the dimeric CsrA/RsmA proteins predominantly hinders ribosome access and translation, which often also reduces the stability of the target RNA (Mercante et al. 2009; Lapouge et al. 2013; Dubey et al. 2005). However, in several cases, CsrA/RsmA protein binding prevents the formation of translation-blocking RNA structures or hinders access of RNases leading to an increase of the total translational efficiency and transcript stability (Ren et al. 2014; Yakhnin et al. 2013). CsrA/RsmA protein activity can be immediately inhibited through sequestration of CsrA by certain non-coding RNAs (e.g., CsrB and CsrC in Enterobacteriaceae), which harbor multiple GGA-containing hairpins. Alternatively, CsrA can be inactivated by binding to specific highly abundant GGA-rich mRNAs as well as by interacting proteins (Kusmierek and Dersch 2017).
CsrA/RsmA deficiency impairs synthesis and function of several T3SSs implicated in motility, host colonization and host defense and strongly attenuates virulence. For instance, CsrA induces the expression of the master regulator FlhDC of the flagellar T3SS in E. coli (Yakhnin et al. 2013). CsrA activates flhDC expression by protecting the flhDC mRNA from decay. mRNA degradation studies in E. coli support a model in which CsrA binding activates flhDC expression by inhibiting the 5′ end-dependent RNase E cleavage pathway (Yakhnin et al. 2013). In addition, the synthesis of the LEE-encoded T3SS for the formation of the intimate attachment structures by EPEC/EHEC is regulated by CsrA on multiple levels (Fig. 3) (Katsowich et al. 2017; Bhatt et al. 2009). First, CsrA directly activates expression of the escD and the LEE4 genes and represses expression of several LEE operons through the regulator Ler and GrlA (Bhatt et al. 2009). Moreover, CsrA was found to interact with the T3SS effector chaperone CesT when it is released from its effector under effector-secreting conditions. Sequestration of CsrA by CesT relieves CsrA-mediated repression of nleA/espI effector mRNA translation, which enables the bacteria to adjust T3SS gene expression in response to host cell contact (Katsowich et al. 2017).
The CsrA equivalent RsmA protein of P. aeruginosa is also implicated in the bacterial response to host cell contact, but the underlying molecular mechanism is quite different. In this pathogen, RsmA controls the expression of the major T3SS transcriptional activator ExsA. The activity of ExsA is controlled by a complex ‘partner-switching’ cascade involving ExsE, ExsC and ExsD, which is triggered upon host cell contact and secretion of the ExsE effector (Fig. 4, for details see Sect. 4.1) (Intile et al. 2014; Dasgupta et al. 2004; Urbanowski et al. 2005). RsmA activity itself is regulated through the magnesium transporter MgtE and the GacAS two-component system via activation of the Csr/Rsm-type RNAs RsmY and RsmZ (Chakravarty et al. 2017).
CsrA has also a very strong impact on the expression of different virulence-relevant T3SSs in Yersinia. Similar to E. coli, CsrA activates the FlhDC master regulator of the flagellar T3SS and is thus required for Yersinia motility (Heroven et al. 2008). Recent work further demonstrates that CsrA has a major influence on the virulence plasmid-encoded T3SS (Ysc/Yop). Expression of the CsrB and CsrC RNAs in Y. pseudotuberculosis is downregulated in the Peyer’s patches during acute infection (Nuss et al. 2017), suggesting that more active CsrA protein is required for virulence. In fact, a csrA-deficient mutant of Yersinia enterocolitica was characterized by reduced secretion of the T3SS effectors YopE and YopH, and a Y. pseudotuberculosis csrA mutant was unable to secrete all known Yop effectors, which are usually injected into neutrophils and macrophages to prevent their phagocytic attack (Nuss et al. 2017; Ozturk et al. 2017). In addition to the virulence plasmid-encoded T3SS, Y. enterocolitica harbors a second chromosomally encoded T3SS (Ysa). This T3SS is only expressed under very special environmental conditions in vitro and seems to promote intracellular virulence (Bent et al. 2015). This Ysa T3SS system is also influenced by CsrA, but in contrast to the Ysc/Yop T3SS effectors, Ysp effector proteins are over-secreted in the csrA mutant (Ozturk et al. 2017).
Similar to Yersinia, CsrA also controls the virulence-associated T3SS of Salmonella typhimurium: the cell invasion-promoting T3SS-1, encoded on SPI-1, and the T3SS-2 mediating Salmonella replication within macrophages (Fig. 1). CsrA regulates the expression of the common regulator HilD by binding near the ribosome binding site on the hilD transcript leading to a decrease of HilD translation and a reduced stability of the hilD mRNA (Altier et al. 2000; Martinez et al. 2011).
3.2 Control of T3SS mRNA Structures and Stability—Influence of Helicases and RNases
The overall efficiency of mRNA translation depends on the stability and the structure of the transcript. Bacteria generally have several RNA helicases that unfold intrinsic hairpin and other secondary RNA structures. Of special interest here is a certain class of RNA-binding helicases, the DEAD-box helicases. They are named after their conserved DEAD amino acid sequence in their catalytic domain and can hydrolyze ATP to dissolve inhibitory duplex RNA structures. One of a set of seven DEAD-box helicases, the DeaD helicase, stimulates translation of the T3SS master regulator ExsA in P. aeruginosa to promote expression of the injectisome (Intile et al. 2015). DeaD seems to directly stimulate exsA mRNA translation, as DeaD-dependent activation is specific to the exsA coding region and the native RBS. The purified protein is able to promote ExsA synthesis using in vitro translation assays (Intile et al. 2015). RNA secondary structure predictions of the 5′-UTR of exsA and the proximal coding sequence revealed extensive base pairing with the RBS, indicating that DeaD enhances ribosomal access. DeaD does not alter T3SS expression through RsmA (Intile et al. 2015), but whether DeaD and RsmA function independently or are dependent upon each other is currently unknown.
Both T3SS regulators and structural components are also targeted by different RNases. One important RNase implicated in T3SS regulation is the polynucleotide phosphorylase (PNPase). PNPase belongs to the group of 3′-exoribonucleases. It can act alone or it functions as part of the multicomponent degradosome complex together with RNase E, the glycolytic enzyme enolase and helicase RhlB (Mohanty and Kushner 2016). In Yersinia, optimal functioning of the virulence plasmid-encoded T3SS was shown to require PNPase. While a pnp deletion mutant of Y. pseudotuberculosis possessed enhanced levels of the T3SS-encoding transcripts and proteins in contrast to wildtype, secretion of the Yop effectors was strongly reduced (Rosenzweig et al. 2007). However, this is in contrast with initial results of our laboratory in which both T3SS gene transcription and Yop secretion was strongly increased in the absence of PNPase in Y. pseudotuberculosis (Kusmierek et al., unpublished). The reason for this discrepancy is unclear, and we are currently testing whether a different genetic background or differences in the growth conditions may be responsible for this discrepancy. It was further found by Rosenzweig et al. that normal T3SS activity was restored when a 70 amino acid peptide (S1 domain) containing one of the RNA-binding domains of PNPase was expressed in the pnp mutant. Notably, T3SS expression, but not T3SS activity, was identical in Δpnp strains expressing active or inactive S1 variants, indicating that PNPase influence on T3SS may involve an RNA intermediate (Rosenzweig et al. 2005, 2007; Rosenzweig and Chopra 2013). Likewise, T3SS functioning is impaired in Y. pseudotuberculosis with a reduced RNase E activity, and these bacteria further resemble the pnp mutant, indicating that they act via a common pathway, e.g., via the degradosome (Yang et al. 2008). In Yersinia, the single-strand-specific RNase Y (YbeY) processing 3′-ends of the 16S RNA was also found to control T3SS expression (Leskinen et al. 2015). The precise mechanism is unknown, but the CsrB and CsrC RNAs are among its target, indicating that the influence of YbeY on T3SS occurs through regulation of the Csr system.
S. typhimurium strains harboring a deletion of the 310 nt 3′-untranslated region (3′-UTR) of hilD or lacking the RNase E gene rne or the PNPase gene pnp exhibit increased hilD mRNA levels. This resulted in SPI-1 gene overexpression, impaired Salmonella growth and uncontrolled invasion of epithelial cells, suggesting that the hilD 3′-UTR is a target for degradation by the bacterial degradosome (Fig. 1) (Lopez-Garrido et al. 2014). In contrast, the RNA chaperone Hfq interacts with the 3′-UTR of the hilD mRNA and has a positive influence on its stability. Therefore, it has been assumed that this effect occurs through competitive inhibition of the degradosome (Lopez-Garrido et al. 2014; Sittka et al. 2007; Chao et al. 2012).
The degradosome is also implicated in the regulation of T3SS gene expression in pathogenic E. coli. In EHEC, the espADB translocon genes are controlled by an RNase E-dependent mechanism, in which a small six-codon mini-open reading frame at the 5’-end of the common transcript is recognized and preferentially degraded by RNase E (Fig. 3). However, translation of the mini-open reading frame by ribosomes protects the mRNA and allows a more efficient production of the translocon proteins (Lodato et al. 2012, 2017).
3.3 Regulatory RNAs
Over the past years, a plethora of regulatory RNAs have been identified in many bacterial pathogens that are implicated in virulence regulation. Besides the Csr/Rsm-type RNAs (see also Sect. 3.1.2), several others of them have also been found to control T3SSs. For instance, the small non-coding RNA Spot42 regulates the expression of the chaperone protein VP1682 of components of the T3SS-1 of Vibrio parahaemolyticus by basepairing with the RBS and the initial codons of the vp1682 transcript (Tanabe et al. 2015). Another example constitutes the Yersinia-specific non-coding RNA Ysr141. In the absence of Ysr141, a selection of the T3SS components and the effectors YpkA, YscF, YopE, YopK and YopJ and the regulator LcrF were 30–70% decreased (Schiano et al. 2014). Although the molecular mechanism how Ysr141 exerts this effect is largely unknown, initial experiments demonstrated that Ysr141 interferes with yopJ mRNA translation. Schiano et al. (Schiano et al. 2014) proposed that all observed changes could be based on the dysregulation of YopJ production as Yersinia T3SS was shown to be sensitive to changes in Yop protein levels. However, the observed regulatory influence on YopJ translation was rather small suggesting that other mechanisms contribute to the overall influence of Ysr141 on T3SS regulation. A recent study revealed that the copy number of the Yersinia virulence plasmid pYV encoding the Ysc/Yop T3SS increases during infection (Wang et al. 2016). This upregulation is caused by an increased expression of the pYV replicase RepA. It was shown that levels of an antisense RNA, CopA, overlapping with the upstream region of the repA gene are strongly decreased under secretion conditions and during infection, leading to a marked decrease of the CopA/repA mRNA ratio and an increase of the copy number (Nuss et al. 2017; Wang et al. 2016). The precise regulatory mechanism still needs to be elucidated, but first evidence exists that the secreted translocon protein YopD is involved in this process (Wang et al. 2016). Finally, the unique bacterial translational control system, including the small protein B (SmpB) and the regulatory RNA SsrA/tmRNA, is required for efficient expression of Yop effectors and the flagellar T3SS of Yersinia (Okan et al. 2006).
A study by Gruber and Sperandio (2015) identified multiple non-coding EHEC-specific RNAs of which sRNA56, sRNA103 and sRNA350 activate T3SS genes of the LEE pathogenicity island (Fig. 3). sRNA350, encoded in the 3′-UTR of the cesF transcript, activates all LEE operons via its influence on the master regulator gene ler, whereas sRNA56 and sRNA103 target only the LEE4-encoded espA mRNA. Besides these EHEC-specific non-coding RNAs, the well-characterized, paralogous non-coding RNAs GlmZ and GlmY also influence expression of EHEC T3SS genes (Fig. 3). Both RNAs destabilize the LEE4- and LEE5-encoded mRNAs and increase translation of the espF transcript (Gruber and Sperandio 2014). GlmZ interacts with the LEE4 mRNA and selectively destabilizes the downstream part of the transcript encoding the translocon espADB genes, but not the upstream part encoding sepL, which acts as regulatory switch by binding effectors until the T3SS is formed (Gruber and Sperandio 2014). In addition, GlmY also represses LEE4 on the post-transcriptional level. However, this occurs by binding to and sequestering the protein RapZ from GlmZ, which, when released from GlmZ, can destabilize the LEE4 transcript (Gruber and Sperandio 2015). The antagonistic control of LEE4/LEE5 and espF by both RNAs is not easy to interpret, as all targeted genes are required for pedestal and A/E lesion formation. However, as suggested by the authors, it is possible that GlmY/GlmZ limits overexpression of the LEE4/LEE5 T3SS components and synchronizes their production with the non-LEE espF gene to enable a precise ratio of the structure components and secreted effectors (Gruber and Sperandio 2014). Moreover, a cis-encoded antisense RNA (Arl) located downstream of the ler gene, covering the last codons and the 3′-UTR, controls T3SS gene expression from the LEE pathogenicity island (Tobe et al. 2014). Interaction of Arl with the ler transcript destabilizes the LEE1 mRNA and also hinders final elongation of the Ler protein synthesis.
3.4 Feedback Control Mechanisms Through Secreted Effectors or Anti-sigma Factors
T3SS gene expression in several pathogens is strongly induced upon host cell contact and effector secretion. This includes the T3SS systems of Yersinia, Salmonella, Shigella and Pseudomonas (Pettersson et al. 1996; Brutinel and Yahr 2008; Zierler and Galan 1995). In Yersinia, T3SS gene expression is coupled to secretion via the translocon protein YopD, the YopD chaperone LcrH and the effector LcrQ (YscM1/YscM2 in Y. enterocolitica) (Anderson et al. 2002; Anderson and Schneewind 1999). LcrQ and YopD are secreted upon host cell contact reducing their concentration in the bacterial cytoplasm. The role of LcrQ is still unclear, but it is assumed that it assists the YopD–LcrH complex (Cambronne and Schneewind 2002; Li et al. 2014). In addition, to its translocon function, YopD is able to interact with RNA (alone or in complex with the chaperone LcrH) by for example binding to the 5′-UTR of multiple yop transcripts and the lcrF mRNA (Fig. 2) (Cambronne and Schneewind 2002; Chen and Anderson 2011). Absence of the YopD protein under secretion conditions strongly decreases their degradation and/or prevents their translation (Chen and Anderson 2011). The RNA-binding mode of the protein is not known, but AU-rich regions in the proximity of the RBS seem important for YopD-mediated repression of the targeted T3SS mRNAs. Another important information shedding more light on the molecular mechanism of cell contact-mediated induction of T3SS genes was obtained by an analysis of Kopaskie et al. (2013). They report that the YopD protein is able to interact with the 30S particles of the bacterial ribosome in an LcrH-dependent manner and could show that YopD in association with YscM1 and LcrH is able to repress YopQ translation. However, how YopD–LcrH interaction with the 30S ribosomal particle is mediated and how this influences the translation of other transcripts of the Ysc/Yop T3SS is still unclear. Yet, it is likely that transient interaction perturbs the formation of the 30S complex before the 50S ribosomal particle associate with the transcript, as no binding of YopD to the assembled 70S ribosome could be detected (Kopaskie et al. 2013).
Another sophisticated feedback control mechanism is promoted by secreted anti-sigma factors and was found for the flagellar T3SS and virulence-associated T3SSs, e.g., from Bordetella spp. (Chevance and Hughes 2017; Ahuja et al. 2016). The flagellar master regulator FlhDC activates fliA, encoding the alternative sigma factor σ28. This sigma factor promotes expression of the motor force generator and the filament, and its function is inhibited when bound by an anti-σ28 factor (FlgM). Upon formation of the hook basal body, the anti-sigma factor is secreted and σ28 is released to activate σ28 target genes (Chevance and Hughes 2017). Similarly, the secreted antagonist BtrA of the sigma factor BtrS establishes a feedback loop that couples the activity of the T3SS with expression of the T3SS genes. BtrA differentially controls nearly 300 genes, including many T3SS genes, which define six distinct regulatory virulence modules in Bordetella (Ahuja et al. 2016).
4 T3SS Regulation on the Protein Level
4.1 Changing Binding Partners
Another mechanism promoting cell contact- and secretion-induced T3SS gene expression is ‘partner-switching.’ One important control step of this process is the interaction of a T3SS chaperone with its T3SS substrate or a cytoplasmic regulatory factor. Without host cell contact, the secreted T3SS effector remains bound to its chaperone that keeps the substrate in a transport-competent stage and inhibits the activating function of the chaperone (Schulmeyer and Yahr 2017). Upon host cell contact, the chaperone is released from the secreted binding partner (effector or translocon proteins) and interacts with transcriptional activators or suppressors of the transcriptional activators (anti-repressor) to induce T3SS gene transcription. This changing of partner(s) can implicate multiple co-, anti- or anti-anti-activators that form a complex feedback control cascade linking T3SS gene expression with the secretory activity of the system (Dasgupta et al. 2004; Urbanowski et al. 2005). This partner-switching mechanism was characterized in detail in P. aeruginosa by the Yahr group and was shown to include four different proteins (Urbanowski et al. 2005; Schulmeyer and Yahr 2017; Vakulskas et al. 2009). In the absence of host cell contact, the effector protein ExsE interacts with chaperone ExsC. The master T3SS transcriptional activator ExsA is bound to ExsD. Upon cell contact, the released ExsC chaperone, which has a higher affinity to ExsD than ExsA, sequesters the ExsD protein, whereby the ExsA activator is liberated and can activate T3SS gene transcription (Brutinel et al. 2010; Zheng et al. 2007; McCaw et al. 2002; Rietsch et al. 2005; Dasgupta et al. 2006). Interestingly, Vibrio parahaemolyticus and Vibrio cholerae appear to have functional orthologues of their Pseudomonas counterparts to control the T3SS-1 (Zhou et al. 2010). A similar mechanism with a very different set of partners has been identified in S. flexneri. In this pathogen, the translocon proteins IpaB and IpaC are bound by the chaperone IpgC. The activator MxiE is inactivated through interaction with the anti-activator OspD1 and Spa15 protein, which acts as OspD1 chaperone under non-secretion conditions. IpaB, IpaC and OspD1 translocation into host cell allows released MxiE and IpgC to interact and activate T3SS gene expression (Parsot et al. 2005).
4.2 Modulation or Modification of T3SS Regulatory Components
Besides interaction with other regulatory proteins, activity of T3SS master regulators can be manipulated either by small compounds or through modification, such as phosphorylation. An exciting recent work demonstrated that long-chain fatty acids (e.g., oleate) prevent expression of the T3SS-1 genes in S. enterica. This inhibition is independent of the long-chain fatty acid degradation pathway and occurs solely through direct binding and inhibition of the DNA-binding activity of the T3SS activator HilD (Golubeva et al. 2016). Long-chain fatty acids are present in the intestinal tract and inhibit HilD-mediated T3SS gene expression until the bacteria reach the distal ileum of the small intestine. There, the metabolites are absorbed and the concentration falls below a critical threshold, which relieves the blockage in order to activate T3SS gene expression.
Another mechanism used to change the activity of T3SS regulators is through protein modification, i.e., tyrosine phosphorylation. However, only a few examples are known, and how the modification influences the activity of the modified proteins is often unclear. One example is Shigella, in which the second master regulator VirB (besides MxiE) is unable to stimulate T3SS gene expression when phosphorylated at residue 247 (Standish et al. 2016).
5 Conclusions and Future Perspectives
The long list of transcriptional, post-transcriptional and post-translational control mechanisms implicated in T3SS control in the different pathogens illustrates that T3SS regulation is highly complex. A large intervening network has been evolved that integrates various environmental signals, nutrient/ion availability and physiological conditions to control regulators, structural components and secreted effectors of the T3SS in a fine-tuned and concerted manner. This occurs through a plethora of sensory and regulatory factors, which can be RNA or proteins that modulate specifically or globally, and the players in the network can be modulated on different regulatory levels.
It is evident, that common players, e.g., conserved AraC/XylS regulators and transcriptional modulators, sensory and regulatory RNA elements, RNases, and common two-component systems are part of the control circuit. However, their interactions, targets and arrangements within the regulatory cascades and feedback cycles can vary significantly between the different pathogens. Moreover, even very small changes in the genetic information were found to provoke fundamental changes of T3SS control. This set of possible variations defines the different T3SS control variants, which adapt and optimize the expression of the secretion system to the distinct needs and lifestyles of the different pathogens.
Ongoing discovery of new regulatory factors and different T3SS control variants further illustrates that our understanding of T3SS regulation is still far from being complete. There is a dire need to explore the molecular mechanisms and the role of regulatory RNAs, controlled RNA degradation and translation changes under non-inducing and secretion conditions during the infection. However, this is challenging due to the complexity of the controlling signals and components. One major difficulty in the analysis of T3SS expression is the identification of appropriate in vitro growth conditions mimicking the different steps of T3SS production under infection conditions.
Another unsolved question is, how the detected molecular mechanisms of one representative strain extend to other strains or members of the family or species. In particular, post-transcriptional control elements such as sensory and regulatory RNAs appear more malleable to intrinsic changes and regulatory rewiring than transcriptional regulators. This promotes individual, strain-specific variations—a trait that is particularly advantageous for the bacteria to adapt to frequently changing host niches. Thus, it would be ill-advised to automatically extrapolate their role to others. For instance, it is known that GlmY/GlmZ promoted control of espF expression, which is essential for EHEC to form pedestals, is not encoded in the genome of closely related EPEC, and the DsrA RNA that activates transcription of ler in EHEC does not affect LEE in EPEC (Bhatt et al. 2016). Moreover, Hfq has a very strong influence on the Ysc/Yop T3SS in Yersinia pestis, but not in Y. enterocolitica, suggesting that T3SS regulation relies on different post-transcriptional mechanisms (Kakoschke et al. 2014, 2016; Schiano et al. 2010). Consequently, the function of these control elements must be experimentally investigated in additional members of the species and family.
An additional future challenge is to unravel the dynamics of the multicomponent and multilayered network of T3SS regulation during different phases of the process. This includes the transition from the repressed stage (e.g., 25 °C, outside host), to the preparing phase (host entry, 37 °C), and the different secretion phases upon host cell contact that allows the bacteria to carefully balance nutrient and energy use to maintain their biological fitness and competiveness.
References
Ahuja U, Shokeen B, Cheng N, Cho Y, Blum C, Coppola G et al (2016) Differential regulation of type III secretion and virulence genes in Bordetella pertussis and Bordetella bronchiseptica by a secreted anti-sigma factor. Proc Natl Acad Sci USA 113(9):2341–2348. https://doi.org/10.1073/pnas.1600320113. PubMed PMID: 26884180; PubMed Central PMCID: PMCPMC4780644
Altier C, Suyemoto M, Lawhon SD (2000) Regulation of Salmonella enterica serovar typhimurium invasion genes by csrA. Infect Immun 68(12):6790–6797. PubMed PMID: 11083797
Anderson DM, Schneewind O (1999) Yersinia enterocolitica type III secretion: an mRNA signal that couples translation and secretion of YopQ. Mol Microbiol 31(4):1139–1148. PubMed PMID: 10096081
Anderson DM, Ramamurthi KS, Tam C, Schneewind O (2002) YopD and LcrH regulate expression of Yersinia enterocolitica YopQ by a posttranscriptional mechanism and bind to yopQ RNA. J Bacteriol 184(5):1287–1295. PubMed PMID: 11844757; PubMed Central PMCID: PMC134855
Bent ZW, Poorey K, Brazel DM, LaBauve AE, Sinha A, Curtis DJ et al (2015) Transcriptomic analysis of Yersinia enterocolitica Biovar 1B infecting murine macrophages reveals new mechanisms of extracellular and intracellular survival. Infect Immun 83(7):2672–2685. https://doi.org/10.1128/iai.02922-14. PubMed PMID: 25895974; PubMed Central PMCID: PMCPMC4468540
Bhatt S, Edwards AN, Nguyen HT, Merlin D, Romeo T, Kalman D (2009) The RNA binding protein CsrA is a pleiotropic regulator of the locus of enterocyte effacement pathogenicity island of enteropathogenic Escherichia coli. Infect Immun 77(9):3552–3568. https://doi.org/10.1128/iai.00418-09. PubMed PMID: 19581394; PubMed Central PMCID: PMCPMC2737987
Bhatt S, Egan M, Jenkins V, Muche S, El-Fenej J (2016) The Tip of the iceberg: on the roles of regulatory small RNAs in the virulence of enterohemorrhagic and enteropathogenic Escherichia coli. Front Cell Infect Microbiol 6:105. https://doi.org/10.3389/fcimb.2016.00105. PubMed PMID: 27709103; PubMed Central PMCID: PMCPMC5030294
Böhme K, Steinmann R, Kortmann J, Seekircher S, Heroven AK, Berger E et al (2012) Concerted actions of a thermo-labile regulator and a unique intergenic RNA thermosensor control Yersinia virulence. PLoS Pathog 8(2):e1002518. Epub 2012/02/24. https://doi.org/10.1371/journal.ppat.1002518. PubMed PMID: 22359501; PubMed Central PMCID: PMC3280987
Brutinel ED, Yahr TL (2008) Control of gene expression by type III secretory activity. Curr Opin Microbiol 11(2):128–133. https://doi.org/10.1016/j.mib.2008.02.010. Epub 2008/04/09. doi:S1369-5274(08)00021-0 [pii]. PubMed PMID: 18396449; PubMed Central PMCID: PMC2387186
Brutinel ED, Vakulskas CA, Yahr TL (2010) ExsD inhibits expression of the Pseudomonas aeruginosa type III secretion system by disrupting ExsA self-association and DNA binding activity. J Bacteriol 192(6):1479–1486. https://doi.org/10.1128/jb.01457-09. PubMed PMID: 20008065; PubMed Central PMCID: PMC2832532
Bustos SA, Schleif RF (1993) Functional domains of the AraC protein. Proc Natl Acad Sci USA 90(12):5638–5642. PubMed PMID: 8516313; PubMed Central PMCID: PMCPMC46776
Büttner D (2012) Protein export according to schedule: architecture, assembly, and regulation of type III secretion systems from plant- and animal-pathogenic bacteria. Microbiol Mol Biol Rev 76(2):262–310. https://doi.org/10.1128/mmbr.05017-11. PubMed PMID: 22688814; PubMed Central PMCID: PMCPMC3372255
Cambronne ED, Schneewind O (2002) Yersinia enterocolitica type III secretion: yscM1 and yscM2 regulate yop gene expression by a posttranscriptional mechanism that targets the 5′ untranslated region of yop mRNA. J Bacteriol 184(21):5880–5893. PubMed PMID: 12374821; PubMed Central PMCID: PMC135404
Chakravarty S, Melton CN, Bailin A, Yahr TL, Anderson GG (2017) Pseudomonas aeruginosa magnesium transporter MgtE inhibits type III secretion system gene expression by stimulating rsmYZ transcription. J Bacteriol 199(23). https://doi.org/10.1128/jb.00268-17. PubMed PMID: 28847924; PubMed Central PMCID: PMCPMC5686585
Chao Y, Papenfort K, Reinhardt R, Sharma CM, Vogel J (2012) An atlas of Hfq-bound transcripts reveals 3’ UTRs as a genomic reservoir of regulatory small RNAs. EMBO J 31(20):4005–4019. https://doi.org/10.1038/emboj.2012.229. PubMed PMID: 22922465; PubMed Central PMCID: PMCPMC3474919
Chen Y, Anderson DM (2011) Expression hierarchy in the Yersinia type III secretion system established through YopD recognition of RNA. Mol Microbiol 80(4):966–980. https://doi.org/10.1111/j.1365-2958.2011.07623.x. Epub 2011/04/13. PubMed PMID: 21481017
Chevance FF, Hughes KT (2017) Coupling of flagellar gene expression with assembly in Salmonella enterica. Methods Mol Biol 1593:47–71. https://doi.org/10.1007/978-1-4939-6927-2_4. PubMed PMID: 28389944
Choi SM, Jeong JH, Choy HE, Shin M (2016)Amino acid residues in the Ler protein critical for derepression of the LEE5 promoter in enteropathogenic E. coli. J Microbiol 54(8):559–564. https://doi.org/10.1007/s12275-016-6027-6. PubMed PMID: 27480636
Dasgupta N, Lykken GL, Wolfgang MC, Yahr TL (2004) A novel anti-anti-activator mechanism regulates expression of the Pseudomonas aeruginosa type III secretion system. Mol Microbiol 53(1):297–308. https://doi.org/10.1111/j.1365-2958.2004.04128.x. PubMed PMID: 15225323
Dasgupta N, Ashare A, Hunninghake GW, Yahr TL (2006) Transcriptional induction of the Pseudomonas aeruginosa type III secretion system by low Ca2+ and host cell contact proceeds through two distinct signaling pathways. Infect Immun 74(6):3334–3341. https://doi.org/10.1128/iai.00090-06. PubMed PMID: 16714561; PubMed Central PMCID: PMCPMC1479281
Deng W, Marshall NC, Rowland JL, McCoy JM, Worrall LJ, Santos AS et al (2017) Assembly, structure, function and regulation of type III secretion systems. Nat Rev Microbiol 15(6):323–337. https://doi.org/10.1038/nrmicro.2017.20. PubMed PMID: 28392566
Diepold A, Wagner S (2014) Assembly of the bacterial type III secretion machinery. FEMS Microbiol Rev 38(4):802–822. https://doi.org/10.1111/1574-6976.12061. PubMed PMID: 24484471
Dorman CJ (2007) H-NS, the genome sentinel. Nat Rev Microbiol 5(2):157–161. https://doi.org/10.1038/nrmicro1598. Epub 2006/12/28. doi:nrmicro1598 [pii]. PubMed PMID: 17191074
Dubey AK, Baker CS, Romeo T, Babitzke P (2005) RNA sequence and secondary structure participate in high-affinity CsrA-RNA interaction. RNA 11(10):1579–1587. https://doi.org/10.1261/rna.2990205. PubMed PMID: 16131593; PubMed Central PMCID: PMCPMC1370842
Ellermeier JR, Slauch JM (2007) Adaptation to the host environment: regulation of the SPI1 type III secretion system in Salmonella enterica serovar Typhimurium. Curr Opin Microbiol 10(1):24–29. https://doi.org/10.1016/j.mib.2006.12.002. PubMed PMID: 17208038
Ellermeier JR, Slauch JM (2008) Fur regulates expression of the Salmonella pathogenicity island 1 type III secretion system through HilD. J Bacteriol 190(2):476–486. https://doi.org/10.1128/jb.00926-07. PubMed PMID: 17993530; PubMed Central PMCID: PMC2223717
Ellermeier CD, Ellermeier JR, Slauch JM (2005) HilD, HilC and RtsA constitute a feed forward loop that controls expression of the SPI1 type three secretion system regulator hilA in Salmonella enterica serovar Typhimurium. Mol Microbiol 57(3):691–705. https://doi.org/10.1111/j.1365-2958.2005.04737.x. PubMed PMID: 16045614
Erhardt M, Dersch P (2015) Regulatory principles governing Salmonella and Yersinia virulence. Front Microbiol 6:949. https://doi.org/10.3389/fmicb.2015.00949. PubMed PMID: 26441883; PubMed Central PMCID: PMCPMC4563271
Francis MS, Wolf-Watz H, Forsberg A (2002) Regulation of type III secretion systems. Curr Opin Microbiol 5(2):166–172. PubMed PMID: 11934613
Galan JE, Lara-Tejero M, Marlovits TC, Wagner S (2014) Bacterial type III secretion systems: specialized nanomachines for protein delivery into target cells. Annu Rev Microbiol 68:415–438. https://doi.org/10.1146/annurev-micro-092412-155725. PubMed PMID: 25002086; PubMed Central PMCID: PMCPMC4388319
Golubeva YA, Ellermeier JR, Cott Chubiz JE, Slauch JM (2016). Intestinal long-chain fatty acids act as a direct signal to modulate expression of the Salmonella Pathogenicity Island 1 type III secretion system. MBio 7(1):e02170–e02175. https://doi.org/10.1128/mbio.02170-15. PubMed PMID: 26884427; PubMed Central PMCID: PMCPMC4752608
Görke B, Stülke J (2008) Carbon catabolite repression in bacteria: many ways to make the most out of nutrients. Nat Rev Microbiol 6(8):613–624. https://doi.org/10.1038/nrmicro1932. PubMed PMID: 18628769
Gruber CC, Sperandio V (2014) Posttranscriptional control of microbe-induced rearrangement of host cell actin. MBio 5(1):e01025-13. https://doi.org/10.1128/mbio.01025-13. PubMed PMID: 24425733; PubMed Central PMCID: PMCPMC3903284
Gruber CC, Sperandio V (2015) Global analysis of posttranscriptional regulation by GlmY and GlmZ in enterohemorrhagic Escherichia coli O157:H7. Infect Immun 83(4):1286–1295. https://doi.org/10.1128/iai.02918-14. PubMed PMID: 25605763; PubMed Central PMCID: PMCPMC4363437
Heroven A, Bohme K, Rohde M, Dersch P (2008) A Csr-type regulatory system, including small non-coding RNAs, regulates the global virulence regulator RovA of Yersinia pseudotuberculosis through RovM. Mol Microbiol 68(5):1179–1195. https://doi.org/10.1111/j.1365-2958.2008.06218.x. Epub 2008/04/24. doi:MMI6218 [pii] . PubMed PMID: 18430141
Hoe NP, Goguen JD (1993) Temperature sensing in Yersinia pestis: translation of the LcrF activator protein is thermally regulated. J Bacteriol 175(24):7901–7909. PubMed PMID: 7504666
Hueck CJ (1998) Type III protein secretion systems in bacterial pathogens of animals and plants. Microbiol Mol Biol Rev 62(2):379–433
Intile PJ, Diaz MR, Urbanowski ML, Wolfgang MC, Yahr TL (2014) The AlgZR two-component system recalibrates the RsmAYZ posttranscriptional regulatory system to inhibit expression of the Pseudomonas aeruginosa type III secretion system. J Bacteriol 196(2):357–366. https://doi.org/10.1128/jb.01199-13. PubMed PMID: 24187093; PubMed Central PMCID: PMCPMC3911257
Intile PJ, Balzer GJ, Wolfgang MC, Yahr TL (2015) The RNA Helicase DeaD stimulates ExsA translation to promote expression of the Pseudomonas aeruginosa type III secretion system. J Bacteriol 197(16):2664–2674. https://doi.org/10.1128/jb.00231-15. PubMed PMID: 26055113; PubMed Central PMCID: PMCPMC4507347
Jackson M, Silva-Herzog E, Plano GV (2004) The ATP-dependent ClpXP and Lon proteases regulate expression of the Yersinia pestis type III secretion system via regulated proteolysis of YmoA, a small histone-like protein. Mol Microbiol 54(5):1364–1378. https://doi.org/10.1111/j.1365-2958.2004.04353.x. Epub 2004/11/24. doi:MMI4353 [pii]. PubMed PMID: 15554975
Kakoschke T, Kakoschke S, Magistro G, Schubert S, Borath M, Heesemann J et al (2014) The RNA chaperone Hfq impacts growth, metabolism and production of virulence factors in Yersinia enterocolitica. PLoS One 9(1):e86113. https://doi.org/10.1371/journal.pone.0086113. PubMed PMID: 24454955; PubMed Central PMCID: PMCPMC3893282
Kakoschke TK, Kakoschke SC, Zeuzem C, Bouabe H, Adler K, Heesemann J et al (2016) The RNA chaperone Hfq is essential for virulence and modulates the expression of four adhesins in Yersinia enterocolitica. Sci Rep 6:29275. https://doi.org/10.1038/srep29275. PubMed PMID: 27387855; PubMed Central PMCID: PMCPMC4937351
Katsowich N, Elbaz N, Pal RR, Mills E, Kobi S, Kahan T et al (2017) Host cell attachment elicits posttranscriptional regulation in infecting enteropathogenic bacteria. Science 355(6326):735–739. https://doi.org/10.1126/science.aah4886. PubMed PMID: 28209897
King JM, Schesser Bartra S, Plano G, Yahr TL (2013) ExsA and LcrF recognize similar consensus binding sites, but differences in their oligomeric state influence interactions with promoter DNA. J Bacteriol 195(24):5639–5650. https://doi.org/10.1128/jb.00990-13. PubMed PMID: 24142246; PubMed Central PMCID: PMC3889609
Kopaskie KS, Ligtenberg KG, Schneewind O (2013) Translational regulation of Yersinia enterocolitica mRNA encoding a type III secretion substrate. J Biol Chem 288(49):35478–35488. https://doi.org/10.1074/jbc.m113.504811. PubMed PMID: 24158443; PubMed Central PMCID: PMC3853294
Kusmierek M, Dersch P (2017) Regulation of host-pathogen interactions via the post-transcriptional Csr/Rsm system. Curr Opin Microbiol 41:58–67. https://doi.org/10.1016/j.mib.2017.11.022. PubMed PMID: 29207313
Laaberki MH, Janabi N, Oswald E, Repoila F (2006) Concert of regulators to switch on LEE expression in enterohemorrhagic Escherichia coli O157:H7: interplay between Ler, GrlA, HNS and RpoS. Int J Med Microbiol 296(4–5):197–210. https://doi.org/10.1016/j.ijmm.2006.02.017. PubMed PMID: 16618552
Lapouge K, Perozzo R, Iwaszkiewicz J, Bertelli C, Zoete V, Michielin O et al (2013) RNA pentaloop structures as effective targets of regulators belonging to the RsmA/CsrA protein family. RNA Biol 10(6):1031–1041. https://doi.org/10.4161/rna.24771. PubMed PMID: 23635605; PubMed Central PMCID: PMCPMC4111731
Leskinen K, Varjosalo M, Skurnik M (2015) Absence of YbeY RNase compromises the growth and enhances the virulence plasmid gene expression of Yersinia enterocolitica O:3. Microbiology 161(Pt 2):285–299. https://doi.org/10.1099/mic.0.083097-0. PubMed PMID: 25416689
Li L, Yan H, Feng L, Li Y, Lu P, Hu Y et al (2014) LcrQ blocks the role of LcrF in regulating the Ysc-Yop type III secretion genes in Yersinia pseudotuberculosis. PLoS One 9(3):e92243. https://doi.org/10.1371/journal.pone.0092243. PubMed PMID: 24658611; PubMed Central PMCID: PMCPMC3962397
Lodato PB, Hsieh PK, Belasco JG, Kaper JB (2012) The ribosome binding site of a mini-ORF protects a T3SS mRNA from degradation by RNase E. Mol Microbiol 86(5):1167–1182. https://doi.org/10.1111/mmi.12050. PubMed PMID: 23043360; PubMed Central PMCID: PMCPMC3537511
Lodato PB, Thuraisamy T, Richards J, Belasco JG (2017) Effect of RNase E deficiency on translocon protein synthesis in an RNase E-inducible strain of enterohemorrhagic Escherichia coli O157:H7. FEMS Microbiol Lett 364(13). https://doi.org/10.1093/femsle/fnx131. PubMed PMID: 28854682
Lopez-Garrido J, Puerta-Fernandez E, Casadesus J (2014) A eukaryotic-like 3’ untranslated region in Salmonella enterica hilD mRNA. Nucleic Acids Res 42(9):5894–5906. https://doi.org/10.1093/nar/gku222. PubMed PMID: 24682814; PubMed Central PMCID: PMC4027200
Madrid C, Nieto JM, Juarez A (2002) Role of the Hha/YmoA family of proteins in the thermoregulation of the expression of virulence factors. Int J Med Microbiol 291(6–7):425–432. PubMed PMID: 11890540
Madrid C, Balsalobre C, Garcia J, Juarez A (2007) The novel Hha/YmoA family of nucleoid-associated proteins: use of structural mimicry to modulate the activity of the H-NS family of proteins. Mol Microbiol 63(1):7–14. PubMed PMID: 17116239
Martinez LC, Yakhnin H, Camacho MI, Georgellis D, Babitzke P, Puente JL et al (2011) Integration of a complex regulatory cascade involving the SirA/BarA and Csr global regulatory systems that controls expression of the Salmonella SPI-1 and SPI-2 virulence regulons through HilD. Mol Microbiol 80(6):1637–1656. https://doi.org/10.1111/j.1365-2958.2011.07674.x. PubMed PMID: 21518393; PubMed Central PMCID: PMC3116662
McCaw ML, Lykken GL, Singh PK, Yahr TL (2002) ExsD is a negative regulator of the Pseudomonas aeruginosa type III secretion regulon. Mol Microbiol 46(4):1123–1133. PubMed PMID: 12421316
Mercante J, Edwards AN, Dubey AK, Babitzke P, Romeo T (2009) Molecular geometry of CsrA (RsmA) binding to RNA and its implications for regulated expression. J Mol Biol 392(2):511–528. https://doi.org/10.1016/j.jmb.2009.07.034. PubMed PMID: 19619561; PubMed Central PMCID: PMC2735826
Miller HK, Kwuan L, Schwiesow L, Bernick DL, Mettert E, Ramirez HA et al (2014) IscR is essential for Yersinia pseudotuberculosis type III secretion and virulence. PLoS Pathog 10(6):e1004194. https://doi.org/10.1371/journal.ppat.1004194. PubMed PMID: 24945271; PubMed Central PMCID: PMC4055776
Mohanty BK, Kushner SR (2016)Regulation of mRNA decay in bacteria. Annu Rev Microbiol 70:25–44. https://doi.org/10.1146/annurev-micro-091014-104515. PubMed PMID: 27297126
Navarre WW, Porwollik S, Wang Y, McClelland M, Rosen H, Libby SJ et al (2006) Selective silencing of foreign DNA with low GC content by the H-NS protein in Salmonella. Science 313(5784):236–238. PubMed PMID: 16763111
Nuss AM, Beckstette M, Pimenova M, Schmühl C, Opitz W, Pisano F et al (2017) Tissue dual RNA-seq: a fast discovery path for infection-specific functions and riboregulators shaping host-pathogen transcriptomes. Proc Natl Acad Sci USA 114(5):E791–E800
Okan NA, Bliska JB, Karzai AW (2006) A Role for the SmpB-SsrA system in Yersinia pseudotuberculosis pathogenesis. PLoS Pathog 2(1):e6. https://doi.org/10.1371/journal.ppat.0020006. Epub 2006/02/02. PubMed PMID: 16450010; PubMed Central PMCID: PMC1358943
Olekhnovich IN, Kadner RJ (2007) Role of nucleoid-associated proteins Hha and H-NS in expression of Salmonella enterica activators HilD, HilC, and RtsA required for cell invasion. J Bacteriol 89(19):6882–6890. https://doi.org/10.1128/jb.00905-07. PubMed PMID: 17675384; PubMed Central PMCID: PMC2045230
Ozturk G, LeGrand K, Zheng Y, Young GM (2017) Yersinia enterocolitica CsrA regulates expression of the Ysa and Ysc type 3 secretion system in unique ways. FEMS Microbiol Lett 364(20). https://doi.org/10.1093/femsle/fnx204. PubMed PMID: 29044402
Parsot C, Ageron E, Penno C, Mavris M, Jamoussi K, d’Hauteville H et al (2005) A secreted anti-activator, OspD1, and its chaperone, Spa15, are involved in the control of transcription by the type III secretion apparatus activity in Shigella flexneri. Mol Microbiol 56(6):1627–1635. https://doi.org/10.1111/j.1365-2958.2005.04645.x. PubMed PMID: 15916611
Pettersson J, Nordfelth R, Dubinina E, Bergman T, Gustafsson M, Magnusson KE et al (1996) Modulation of virulence factor expression by pathogen target cell contact. Science 273(5279):1231–1233
Poncet S, Milohanic E, Maze A, Abdallah JN, Ake FML et al (2009) Correlations between carbon metabolism and virulence in bacteria. Contrib Microbiol 16:88–102
Portaliou AG, Tsolis KC, Loos MS, Zorzini V, Economou A (2016) Type III secretion: building and operating a remarkable nanomachine. Trends Biochem Sci 41(2):175–189. https://doi.org/10.1016/j.tibs.2015.09.005. PubMed PMID: 26520801
Ren B, Shen H, Lu ZJ, Liu H, Xu Y (2014) The phzA2-G2 transcript exhibits direct RsmA-mediated activation in Pseudomonas aeruginosa M18. PLoS One 9(2):e89653. https://doi.org/10.1371/journal.pone.0089653. PubMed PMID: 24586939; PubMed Central PMCID: PMCPMC3933668
Rhigetti F, Nuss AM, Twittenhoff C, Beele S, Urban K, Will S et al (2016) Temperature-responsive in vitro RNA structurome of Yersinia pseudotuberculosis. Proc Natl Acad Sci 113(26):7237–7242
Rietsch A, Vallet-Gely I, Dove SL, Mekalanos JJ (2005) ExsE, a secreted regulator of type III secretion genes in Pseudomonas aeruginosa. Proc Natl Acad Sci USA 102(22):8006–8011. https://doi.org/10.1073/pnas.0503005102. PubMed PMID: 15911752; PubMed Central PMCID: PMCPMC1142391
Rosenzweig JA, Chopra AK (2013) The exoribonuclease polynucleotide phosphorylase influences the virulence and stress responses of yersiniae and many other pathogens. Front Cell Infect Microbiol 3:81. https://doi.org/10.3389/fcimb.2013.00081. PubMed PMID: 24312901; PubMed Central PMCID: PMCPMC3832800
Rosenzweig JA, Weltman G, Plano GV, Schesser K (2005) Modulation of Yersinia type three secretion system by the S1 domain of polynucleotide phosphorylase. J Biol Chem 280(1):156–163. https://doi.org/10.1074/jbc.m405662200. PubMed PMID: 15509583
Rosenzweig JA, Chromy B, Echeverry A, Yang J, Adkins B, Plano GV et al (2007) Polynucleotide phosphorylase independently controls virulence factor expression levels and export in Yersinia spp. FEMS Microbiol Lett 270(2):255–264. https://doi.org/10.1111/j.1574-6968.2007.00689.x. PubMed PMID: 17391372
Schiano CA, Bellows LE, Lathem WW (2010) The small RNA chaperone Hfq is required for the virulence of Yersinia pseudotuberculosis. Infect Immun 78(5):2034–2044. https://doi.org/10.1128/iai.01046-09. PubMed PMID: 20231416; PubMed Central PMCID: PMC2863511
Schiano CA, Koo JT, Schipma MJ, Caulfield AJ, Jafari N, Lathem WW (2014) Genome-wide analysis of small RNAs expressed by Yersinia pestis identifies a regulator of the Yop-Ysc type III secretion system. J Bacteriol 196(9):1659–1670. Epub 2014/02/18. https://doi.org/10.1128/jb.01456-13. PubMed PMID: 24532772; PubMed Central PMCID: PMC3993326
Schleif R (2010) AraC protein, regulation of the l-arabinose operon in Escherichia coli, and the light switch mechanism of AraC action. FEMS Microbiol Rev 34(5):779–796. https://doi.org/10.1111/j.1574-6976.2010.00226.x. PubMed PMID: 20491933
Schulmeyer KH, Yahr TL (2017) Post-transcriptional regulation of type III secretion in plant and animal pathogens. Curr Opin Microbiol 36:30–36. https://doi.org/10.1016/j.mib.2017.01.009. PubMed PMID: 28189908; PubMed Central PMCID: PMCPMC5534366
Schwiesow L, Lam H, Dersch P, Auerbuch V (2015) Yersinia type III secretion system master regulator LcrF. J Bacteriol 198(4):604–614. https://doi.org/10.1128/jb.00686-15. PubMed PMID: 26644429; PubMed Central PMCID: PMCPMC4751813
Shimizu T, Ichimura K, Noda M (2015) The surface sensor NlpE of enterohemorrhagic Escherichia coli contributes to regulation of the type III secretion system and flagella by the Cpx response to adhesion. Infect Immun 84(2):537–549. https://doi.org/10.1128/iai.00881-15. PubMed PMID: 26644384; PubMed Central PMCID: PMCPMC4730559
Sittka A, Pfeiffer V, Tedin K, Vogel J (2007) The RNA chaperone Hfq is essential for the virulence of Salmonella typhimurium. Mol Microbiol 63(1):193–217. https://doi.org/10.1111/j.1365-2958.2006.05489.x. PubMed PMID: 17163975; PubMed Central PMCID: PMCPMC1810395
Standish AJ, Teh MY, Tran ENH, Doyle MT, Baker PJ, Morona R (2016) Unprecedented abundance of protein tyrosine phosphorylation modulates Shigella flexneri virulence. J Mol Biol 428(20):4197–4208. https://doi.org/10.1016/j.jmb.2016.06.016. PubMed PMID: 27380737
Tanabe T, Miyamoto K, Tsujibo H, Yamamoto S, Funahashi T (2015) The small RNA Spot 42 regulates the expression of the type III secretion system 1 (T3SS1) chaperone protein VP1682 in Vibrio parahaemolyticus. FEMS Microbiol Lett 362(21). https://doi.org/10.1093/femsle/fnv173. PubMed PMID: 26394644
Teixido L, Carrasco B, Alonso JC, Barbe J, Campoy S (2011) Fur activates the expression of Salmonella enterica pathogenicity island 1 by directly interacting with the hilD operator in vivo and in vitro. PLoS One 6(5):e19711. https://doi.org/10.1371/journal.pone.0019711. PubMed PMID: 21573071; PubMed Central PMCID: PMC3089636
Tobe T, Yen H, Takahashi H, Kagayama Y, Ogasawara N, Oshima T (2014 )Antisense transcription regulates the expression of the enterohemorrhagic Escherichia coli virulence regulatory gene ler in response to the intracellular iron concentration. PLoS One 9(7):e101582. https://doi.org/10.1371/journal.pone.0101582. PubMed PMID: 25006810; PubMed Central PMCID: PMCPMC4090186
Urbanowski ML, Lykken GL, Yahr TL (2005) A secreted regulatory protein couples transcription to the secretory activity of the Pseudomonas aeruginosa type III secretion system. Proc Natl Acad Sci USA 102(28):9930–9935. https://doi.org/10.1073/pnas.0504405102. PubMed PMID: 15985546; PubMed Central PMCID: PMC1175016
Vakulskas CA, Brady KM, Yahr TL (2009) Mechanism of transcriptional activation by Pseudomonas aeruginosa ExsA. J Bacteriol 191(21):6654–6664. https://doi.org/10.1128/jb.00902-09. PubMed PMID: 19717612; PubMed Central PMCID: PMC2795306
Vakulskas CA, Potts AH, Babitzke P, Ahmer BM, Romeo T (2015) Regulation of bacterial virulence by Csr (Rsm) systems. Microbiol Mol Biol Rev 79(2):193–224. https://doi.org/10.1128/mmbr.00052-14. PubMed PMID: 25833324
Vergnes A, Viala JP, Ouadah-Tsabet R, Pocachard B, Loiseau L, Meresse S et al (2017) The iron-sulfur cluster sensor IscR is a negative regulator of Spi1 type III secretion system in Salmonella enterica. Cell Microbiol 19(4). https://doi.org/10.1111/cmi.12680. PubMed PMID: 27704705
Wang H, Avican K, Fahlgren A, Erttmann SF, Nuss AM, Dersch P et al (2016) Increased plasmid copy number is essential for Yersinia T3SS function and virulence. Science 353(6298):492–495. https://doi.org/10.1126/science.aaf7501. PubMed PMID: 27365311
Yakhnin AV, Baker CS, Vakulskas CA, Yakhnin H, Berezin I, Romeo T et al (2013) CsrA activates flhDC expression by protecting flhDC mRNA from RNase E-mediated cleavage. Mol Microbiol 87(4):851–866. https://doi.org/10.1111/mmi.12136. PubMed PMID: 23305111; PubMed Central PMCID: PMCPMC3567230
Yang J, Jain C, Schesser K (2008) RNase E regulates the Yersinia type 3 secretion system. J Bacteriol 190(10):3774–3778. https://doi.org/10.1128/jb.00147-08. PubMed PMID: 18359811; PubMed Central PMCID: PMCPMC2395017
Zheng Z, Chen G, Joshi S, Brutinel ED, Yahr TL, Chen L (2007) Biochemical characterization of a regulatory cascade controlling transcription of the Pseudomonas aeruginosa type III secretion system. J Biol Chem 282(9):6136–6142. https://doi.org/10.1074/jbc.m611664200. PubMed PMID: 17197437
Zhou X, Konkel ME, Call DR (2010) Regulation of type III secretion system 1 gene expression in Vibrio parahaemolyticus is dependent on interactions between ExsA, ExsC, and ExsD. Virulence 1(4):260–272. https://doi.org/10.4161/viru.1.4.12318. PubMed PMID: 21178451; PubMed Central PMCID: PMCPMC3073295
Zierler MK, Galan JE (1995) Contact with cultured epithelial cells stimulates secretion of Salmonella typhimurium invasion protein InvJ. Infect Immun 63(10):4024–4028
Author information
Authors and Affiliations
Corresponding author
Editor information
Editors and Affiliations
Rights and permissions
Copyright information
© 2019 Springer Nature Switzerland AG
About this chapter
Cite this chapter
Volk, M., Vollmer, I., Heroven, A.K., Dersch, P. (2019). Transcriptional and Post-transcriptional Regulatory Mechanisms Controlling Type III Secretion. In: Wagner, S., Galan, J. (eds) Bacterial Type III Protein Secretion Systems. Current Topics in Microbiology and Immunology, vol 427. Springer, Cham. https://doi.org/10.1007/82_2019_168
Download citation
DOI: https://doi.org/10.1007/82_2019_168
Published:
Publisher Name: Springer, Cham
Print ISBN: 978-3-030-52122-6
Online ISBN: 978-3-030-52123-3
eBook Packages: Biomedical and Life SciencesBiomedical and Life Sciences (R0)