Skip to main content

Human microbiota modulation via QseC sensor kinase mediated in the Escherichia coli O104:H4 outbreak strain infection in microbiome model

A Correction to this article was published on 24 August 2021

This article has been updated



The intestinal microbiota plays a crucial role in human health, adjusting its composition and the microbial metabolites protects the gut against invading microorganisms. Enteroaggregative E. coli (EAEC) is an important diarrheagenic pathogen, which may cause acute or persistent diarrhea (≥14 days). The outbreak strain has the potent Shiga toxin, forms a dense biofilm and communicate via QseBC two-component system regulating the expression of many important virulence factors.


Herein, we investigated the QseC histidine sensor kinase role in the microbiota shift during O104:H4 C227–11 infection in the colonic model SHIME® (Simulator of the Human Intestinal Microbial Ecosystem) and in vivo mice model. The microbiota imbalance caused by C227–11 infection affected ỿ-Proteobacteria and Lactobacillus spp. predominance, with direct alteration in intestinal metabolites driven by microbiota change, such as Short-chain fatty acids (SCFA). However, in the absence of QseC sensor kinase, the microbiota recovery was delayed on day 3 p.i., with change in the intestinal production of SCFA, like an increase in acetate production. The higher predominance of Lactobacillus spp. in the microbiota and significant augmented qseC gene expression levels were also observed during C227–11 mice infection upon intestinal depletion. Novel insights during pathogenic bacteria infection with the intestinal microbiota were observed. The QseC kinase sensor seems to have a role in the microbiota shift during the infectious process by Shiga toxin-producing EAEC C227–11.


The QseC role in C227–11 infection helps to unravel the intestine microbiota modulation and its metabolites during SHIME® and in vivo models, besides they contribute to elucidate bacterial intestinal pathogenesis and the microbiota relationships.


The human digestive tract hosts hundreds of microorganism’s species that are collectively known as microbiota. The gut microbiota is a complex and dynamic ecosystem that includes bacteria, archaea, virus, fungi and protozoa [1]. The colon albeits the largest and most diverse microbial population in the human intestine, with approximately 1012 bacterial cells per gram of luminal contents [2]. This community is predominantly composed of Firmicutes and Bacteroidetes phyla, followed by Protobacteria and Actinobacteria [3]. The intestinal microbiota composition may influence the functions of the cardiovascular, nervous and endocrine systems [4,5,6]. Moreover, the microbiota provides many benefits for human health such as the development of the digestive and immune systems, production of vitamins, metabolization and availability of nutrients, as well as protection against several pathogens [7, 8]. The balance between commensal and potentially pathogenic bacteria is a central element of human health. Thus, the microbiota dysbiosis may result in greater susceptibility to the development of infectious and chronic diseases [9, 10].

Short-chain fatty acids (SCFA) are the main metabolites from polysaccharide fermentation by anaerobic bacteria in the colon, SCFA such as acetate, propionate and butyrate represent about 90–95% of their composition [11, 12]. SCFA play an important role in maintaining gut health, such as protection, energy source and physiological homeostasis [13]. Acetate is the main SCFA produced in the colon, and also the most abundant in the bloodstream [14, 15]. The acetate activity in the colon has an anti-inflammatory role, it helps the pH balance, increases blood flow and improve oxygen uptake; it is also used as a substrate for the butyrate production by other members of the microbiota during the cross-feeding process [16].

Infectious diarrhea is a major global public health problem, unfortunately it ranks high in mortality rate among all ages, and amongst infants under 5 years old is classified within the top 5 mortality cause [17]. Enteroaggregative E. coli (EAEC) is an important etiologic agent of acute and persistent diarrhea (≥14 days) for both children and adults worldwide [17, 18]. This pathogen is known to produce a thick biofilm and a typical adhesion pattern in cell cultures similar to stacked bricks, mediated mainly by aggregate adhesion fimbriae (AAF). Five variants of this fimbria have been described (AAF/I-V), all of them encoded by pAA plasmid and dependent of the AggR transcriptional regulator, as an activator. AggR has been described in EAEC as an important transcriptional activator of at least 44 virulence genes, such as those encoding AAFs and a dispersin (antiaggregation protein) [19,20,21,22,23,24]. Nonetheless, this pathotype is a genetically very heterogeneous bacterial group, whereas recent studies have found virulence factors statistically correlated with disease, although EAEC complete pathogenesis process remain unclear [25, 26].

In 2011, a large outbreak of foodborne bloody diarrhea began in Germany and quickly spread to other countries, resulting in 3816 sick people and 54 deaths [27]. The O104:H4 strains were immediately sequenced and directly linked to these cases. Interesting most of these strains were Shiga toxin (Stx) type 2 (Stx2) producers, usually found in enterohemorrhagic E. coli (EHEC) and other Shiga toxin-producing E. coli (STEC), utmost related to hemorrhagic colitis (HC) and hemolytic uremic syndrome (HUS) cases. The outbreak strains isolated showed a deadly combination of EAEC virulence factors and Stx2 in these highly virulent strains [28]. The O104:H4 strain C227–11 is the main representative isolate from this outbreak in Europe [29]. Additionally, this strain produces SPATEs (Serine Protease Autotransporters of Enterobacteriaceae) [30, 31], such as Pic, SigA and SepA involved in the infectious niche establishment [29, 30]. Moreover, this C227–11 outbreak strain encodes AAF/I (aggregative adherence fimbriae I), the antiaggregation dispersin, and other important adhesins related to biofilm formation, such as LPF (long polar fimbriae) and Iha (IrgA homologue adhesin) [28, 32].

The coordination of metabolic and pathogenic mechanisms in bacteria are mediated by chemical signaling via 2-component systems, also known as quorum sensing [33]. The QseBC 2-component system, first described in EHEC [34], plays a crucial role in regulating the virulence genes expression of important human enteropathogens [35]. This system is composed by inner membrane histidine kinase sensor QseC and a cytoplasmic response regulator QseB. QseC mediates inter-kingdom signaling by detecting host stress hormones, epinephrine and norepinephrine, in addition to Autoinducer-3, a molecule produced by a diversity of Gram-positive and negative bacteria [34, 36, 37]. In EHEC, QseC detects these environmental signals, and activates the virulence genes transcription of LEE pathogenicity island, motility and Shiga toxin [38]. In addition, QseC homologues are found in at least 25 bacterial pathogens [39]. Recently, its role has been described in the EAEC pathogenicity, whereas the QseC sensor kinase was shown to be important during in vitro and in infection via Type I fimbriae adherence [40,41,42].

There are limitations to the use of animal models to investigate EAEC infection, since the pathogen has multiple virulence features and the models only mimic partially the pathogenesis without diarrhea, as well as ethical limits to conduct clinical trials [43]. Animal models in EAEC such as oral mice infection is employed to mimic the natural oral route, with antibiotic depletion to favour EAEC colonization [44], this model seems very appropriated to compare the intestinal murine colonization in vivo with a reactor in vitro model colonized by human microbiota. Therefore, a colonic model, such as the Simulator of the Human Intestinal Microbial Ecosystem (SHIME®) [45, 46] becomes an excellent tool to correlate the human microbiota and bacterial pathogenesis. This system mimics physiological conditions, such as pH, temperature, transit time, enzymatic digestive activity, and gut microbiota in the gastrointestinal tract [47]. Vast amount and variety of metabolites have been described by gut microbiota, the SCFA are abundant and important energy sources for intestinal colonic cells and microbial population, besides an important role in the host metabolism and immune system homeostasis [48].

The present study has investigated the QseC role in the microbiota shift and metabolites composition in the intestinal microbiome during O104:H4 Stx + outbreak strain infection in the human colonic model SHIME® and mice infection.


QseC sensor kinase modulates human intestinal microbiota shift during C227–11 Stx + infection during SHIME® infection

The QseC sensor kinase role in intestinal microbiota composition was verified during the Shiga toxin producing O104:H4 E.coli infection. The C227–11 and C227–11::qseC strain were employed during in vitro infection of controlled colonic SHIME® model, to mimic the human gastrointestinal tract, evaluating the intestinal microbiota abundance through C227–11 infection [49], as detailed illustrated (Fig. 1a and b). Here, we have analyzed the Firmicutes, Bacteroidetes and ỿ-Proteobacteria phyla presence measuring their levels in the system, as well as the abundance of bacterial genera present in the human intestine as Lactobacillus spp., Bifidobacterium spp., Prevotella spp., and Bacteroides spp. [3, 50]. The viable bacterial cells in the system were measured via qRT-PCR from day 0 to day 3 after C227–11 and C227–11::qseC strains infection. Initially, there was a 30% increase in Bacteroidetes and a 15% decrease in both ỿ-Proteobacteria and Firmicutes during C227–11 strain infection, on day 1 p.i., when compared to day 0. Therefore, the ỿ-Proteobacteria phylum was predominate among the all analyzed phyla here after day 1p.i., whereas it has reached 70 and 96% on days 2 and 3p.i. respectively (Fig. 2a), with consequent decrease in Firmicutes and Bacteroidetes. Specifically, at the genus level, we observed 44% decrease in Bacteroides spp. levels, 49% in Bifidobacterium spp. and a small increase of 8% in Prevotella spp. on day 1 p.i. when compared to day 0. However, Lactobacillus spp. have shown 86% on day 1 and 97% on day 2, reaching higher prevalence on days 2 and 3 p.i. (Fig. 2b). Both WT and C227–11::qseC strain were measured in vitro and have similar growth rates (Supplemental Material, Fig. 1S).

Fig. 1
figure 1

SHIME® infection model overview employed with all controlled containers representing the gastrointestinal tract, with stomach and its feed, small intestine and its pancreatic juice and the ascending colon triplicates employed here. The arrows indicate the flow direction of the pumps, dashed lines for gas and solid lines for liquids (a). Experimental protocol with all period steps developed in 5 weeks during C227–11 infection (b). C227–11 and C227–11::qseC strains presence in output was verified by PCR amplification

Fig. 2
figure 2

Microbiota predominance modulated via QseC during C227–11 infection in the SHIME® model. Relative microbiota abundance analysis via qRT-PCR of 16 s rRNA of phyla and genera. Microbiota composition from days 0 to 3 p.i with strain C227–11 infection, respectively, phyla and genera (a and b), and with strain C227–11::qseC infection, respectively, phyla and genera (c and d). ELISA Immunoassay capture to measure the Stx levels from the output collected during the SHIME® infection, day 1, ** p = 0.002 and 3 p.i., ** p = 0.009 (e). The statistical significance analyzes were performed on GraphPad Prism 7 via t-test

Clearly in the absence of the QseC sensor kinase, the C227–11::qseC strain infection has shown the predominance of ỿ-Proteobacteria with 82 and 71% on day 1 and day 2 p.i. respectively. However, clear decrease was evidenced, with 8% in ỿ-Proteobacteria, followed by 4% of Bacteroides and an incredibly augment to 88% of Firmicutes, all at day 3 p.i. (Fig. 2c). The genera analysis demonstrated only 3% of Lactobacillus sp. on day 1, as well as its gradual increase that reaching 70% on day 2 p.i. and 82% on day 3 p.i., and also showed a low amount of Prevotella spp. and Bacteroides spp. on day 2 (4 and 8%) and on day 3 (1 and 16%) (Fig. 2d). These microbiota fluctuations QseC-dependent may be related to different chemical signals sensed in the SHIME® model.

Next, the SHIME® model was also employed to verify if the C227–11 interaction with the human intestinal microbiota was enough to trigger Shiga toxin expression, measured via ELISA capture immunoassay from fractions collected in the day 1 and 3 p.i.. The Stx levels were higher in the C227–11 strain infection in both days, with decrease observed in the C227–11::qseC strain, respectively in the order of 30 and 40% (Fig. 2e).

Short-chain fatty acids (SCFA) key production by the human gut microbiota

The microbiota-derived SCFAs have important role during pathogenesis since many enteric pathogens have adapted to distinct SCFA gradients and consequently have evolved mechanisms to regulate virulence gene expression [48, 51, 52].

The QseC sensor kinase absence affected directly the microbiota composition to be restored only on day 3 p. i., here we evaluated in the period whether this would also result in differences in the production of the three main SCFAs found in the intestine, acetate, butyrate, propionate (Fig. 3). The SFCA production during SHIME® infection was assessed by measuring it directly via gas chromatography from day 0 to day 3 p.i. The C227–11 strain infection showed a 42.6% decrease in acetate production on day 1 p.i., and no significant difference was observed on the following days, as well as for propionate and butyrate (Figs. 3a and 4a). Gradually, the acetate levels have increased from day 0 to day 3 p.i. during C227–11::qseC strain infection, and a distinguished difference of 18.5 and 39.9% was observed, on days 2 and 3p.i., respectively (Fig. 4b). Propionate production has not shown significant changes; conversely, butyrate production has shown a decreased of 45.4% on day 2 p.i., (*p ≤ 0.0371, ***p < 0.0001, *p < 0.0309) (Figs. 3b and 4b). Distinctly, the acetate was more abundant in the two groups evaluated here, and commonly acetate is the more abundant SCFA in the colon [15].

Fig. 3
figure 3

Direct acetate, propionate and butyrate production analysis (mmol/L) from day 0 to day 3.p.i. via gas chromatography. SCFA composition from C227–11 infection period (a) (*** p = 0.0003) and C227–11::qseC (b). Analyzes were performed individually for each SCFA compared to day 0. The statistical significance analyzes were performed on GraphPad Prism 7 via one-way ANOVA and Tukey post hoc test (*p = 0.0371, *p = 0.0309, *** p = 0.0001)

Fig. 4
figure 4

Percentile balance of acetate, propionate and butyrate occurrence from total SCFA production analysis via gas chromatography, daily kinetics during infection, from 0 to day 3 p.i. Differential occurrence in the C227–11(a) and C227–11::qseC strains (b) infection. Gradient from 0% (blue) to 100% (red) concentration of each SCFA

Interplay between the intestinal microbiota composition and the production of SCFA during the infectious process

The composition and level of SCFA is directly related to the distribution of this gut microbial community [53]. Therefore, we assessed the relationship between the microbiota abundance and the daily percentage of each SCFA. Although changes between phyla and genera were observed during the C227–11 strain experimental period, as seen by the large increase of ỿ-Proteobacteria and Lactobacillus spp. on days 2 and 3 p.i. (Fig. 2a and b), and C227–11::qseC strain showed correlation between the decrease of ỿ-Proteobacteria, especially after day 2 p.i. (Fig. 2c). In addition to Firmicutes increase on day 3p.i., phylum that includes the Lactobacillus genus (Fig. 2c and d). Correspondently to the correlation is observed in bacterial frequency and production of acetate between day 1–3 p.i, increasing both Lactobacillus genus and acetate (Fig. 3). The daily proportion among acetate, propionate and butyrate remains steady without significant changes (Fig. 4a), only a gradual increase in acetate production (Fig. 4b).

QseC sensor kinase also drives the intestinal microbiota shift during C57BL/6 mice infection

We performed in vivo C57BL/6 mice infection to verify and validate the collected data from SHIME® model with a distinct microbiota, together with the virulence features and host response in this model as key components of the mice infection. The genera predominance after infection has shown higher levels of Lactobacillus spp. during C227–11 infection in the days 1 and 3 p.i. when compare to C227–11::qseC strain (Fig. 5a), where Lactobacillus spp. have only increased by day 3 p.i. when compared to Bacteroides sp. and Bifidobacterium spp. The qseC gene expression levels were also higher in strains here tested later during infection of C57BL/6 mice in the day 3 p.i., as the C227–11 and the canonical 042 strain (EAEC pathogenic prototype, O44:H18, Stx), reached 17 and 34-fold change increase, when compared with the control DH5α strain levels in the day 3 p.i., with a lower 6-fold change increase (Fig. 5b), mortality was not observed in the assay employing five (5) mice per group.

Fig. 5
figure 5

Microbiota predominance during C57BL/6 mice infection, C227–11and C227–11::qseC strains (a). Expression levels of qseC during early and later infection (day 1-3p.i.) of C227–11, 042 and DH5α strains, p-values are respectively p =0.006 (**), p = 0.001 (**) and p =0.004 (**) (b). Relative expression levels were measured in vitro of stx2a gene from the C227–11, C227–11::qseC, and C227–11qseC+ (pBAD33 qseC), p =0.01 (**), p =0.001 (***) (c)

The evaluation of the stx gene expression levels was also employed to measure an important virulence factor during in vitro LB growth to evaluate the QseC sensor kinase absence impact and its importance to restore the expression levels when the C227–11::qseC strain was complemented. The stx expression levels are diminished in the C227–11::qseC strain as 2-fold lower than WT levels and restored upon qseC pBAD33 complementation to similar WT levels (Fig. 5c).


The fundamental role of the intestinal microbiota in resistance to colonization by invading pathogens, which involve both direct and indirect mechanisms, the microbiota together with immune system works as essential lines of host defense. The QseBC 2-component system is employed to sense the environment surroundings and regulate the virulence traits in C227–11 E.coli strain and other pathogens, but also to help bacterial colonization and nutrients scavenging [8, 54]. Therefore, it is crucial to understand the intestinal interaction between microbiota and the pathogen during the development of the disease. The QseBC has been shown to be an important way to modulate pathogenic mechanisms of several human enteropathogens, such as EHEC, EAEC, and Salmonella Typhimurim [34, 55], previously changes in the microbiota abundance driven by QseC and QseE have been described in Citrobacter rodentium, a surrogate model for EHEC [56]. Herein, the human colonic intestinal microbiota model was employed to study the chemical signaling influence in the process to better understand the QseC sensor kinase importance in the C227–11 colonization in the SHIME® model and the in vivo model corroborates to drive the microbiota prevalence, that affects the SCFA concentration during infection.

The microbiota imbalance was clear during C227–11 infection in the SHIME® model, upon C227–11 strain infection the Lactobacillus spp. and ỿ-Proteobacteria colonization have augmented (Fig. 2a and b). The higher levels of ỿ-Proteobacteria phylum, which includes Gram-negative bacteria, tends to increase intestinal permeability and trigger the inflammatory process by releasing LPS (lipopolysaccharide), as a bacterial endotoxin. This phylum includes very critical enteropathogens such as E. coli pathotypes, Salmonella, Yersinia, Vibrio and Pseudomonas, thus, its increase may be permissive to human health [57,58,59]. The absence of QseC sensor kinase within the SHIME® model during microbiota interaction seems to attenuate the C227–11 strain upon microbiota interaction, with lower secretion of Shiga toxin noted in the C227–11::qseC than WT strain in the ELISA immunoassay direct assayed from the intestinal extracts (Fig. 2e), the direct link between QseC and Shiga toxin in the C227–11 strain demands further studies. However, the data here raises the point about Shiga toxin possible implication in C227–11 strain during the human intestinal microbiota competition, since the model lacks the presence of host tissue.

The QseC sensor seems to be key player during infection, whereas the C227–11::qseC strain infection in the SHIME® model had delayed recovery of the indigenous microbiota only by day 3 p.i. (Fig. 2c and d). It was also observed high levels of Firmicutes (Fig. 2c), consider as the main bacteriocins producer [60]. Higher abundance of Bacteroides spp. and Bifidobacterium spp. (Fig. 2d) was observed after C227–11::qseC strain infection, both important bacteria to increase the acetate levels [51, 61]. The C227–11::qseC mutant infection has presented a distinct balance of microbiota composition in the SHIME model, this difference is more prominent in the 2 initial days, by day 3 p.i. the differences in composition became less evident. These data imply QseC major role in the initial infection in the SHIME® model. Again, the indigenous intestinal microbiota shows its importance during maintenance of gastrointestinal homeostasis and the host’s intestinal health [62]. Commensal and probiotic intestinal bacteria are important against enteric disease by several mechanisms, including competitive exclusion, adhesion, and production of antimicrobial compounds [63]. There are limitations for in vivo EAEC infection models, since the colonization of these bacteria need a partial microbiota depletion, affecting the intestinal conditions, additionally most of the animal models do not reproduce the diarrheagenic component of the enteropathogens disease. Therefore, the colonic model SHIME® may be employed as important possibility to further investigate the interaction between the pathogen and the human microbiota in conditions similar to intestine in a controlled environment.

Members of the Bacteroidetes phylum, more specifically Bacteroides spp., are primarily responsible for the acetate and propionate production, while members of the Firmicutes phylum, are the main producers of butyrate [64]. However, it is known that members of the four main phyla contribute substantially to the production of SCFA, thus, the imbalance of the intestinal microbiota may result in changes in the production of these metabolites and health disorders [52, 65].

Recently, we have shown that QseBC system signaling pathway interruption has substantially reduced the EAEC colonization and virulence gene expression in mice model of infection of fimH, that encodes de Type I fimbriae pilin and QseC essential role during the in vivo model to modulate the microbiota imbalance at Phyla level in mice during EAEC infection [42]. Nonetheless, similar studies have evidenced QseC importance during the Citrobacter rodentium infection, a natural pathogen of mice that mimics EHEC infection in vivo, the reduction of colonization and virulence factors expression such as espA and tir, in addition to decrease the ỿ-Proteobacteria levels [56]. The data presented here indicate how the pathogens such as C227–11 may play a role in the intestinal microbiota balance, therefore contribute to microbiota composition and abundance of distinct intestinal bacteria and metabolites as direct effect caused by the pathogen presence (Figs. 2, 3 and 4).

The SCFA adequate levels in the intestine are important for human health, because they perform vital functions for the gastrointestinal system [66]. In additional, the SCFAs have an important role during EHEC pathogenesis, because they impact EHEC gene regulation. Butyrate works as a signal in EHEC by enhancing the expression of the T3SS and flagellar genes [67]. Here, the C227–11 strain infection have shown significant change in the SCFA levels, such as 42% decrease in acetate production on day 1 p.i. (Fig. 3a). Probably, the QseC histidine kinase sensor absence in the C227–11 mutant strain contributed to a positive microbiota modulation during infection period, and to increased acetate production (Fig. 3b).

Previously work with these metabolites have also shown that they may cross the bacterial membrane and accumulate in the cytoplasm, leading to the influx of protons and consequent intracellular acidification [52].. Higher levels of acetate produced by Bifidobacteria spp. were correlated with protection against EHEC O157:H7 infection in mice. Moreover, acetate prevented the decreases in transepithelial electrical resistance, which contributes to lower translocation of Shiga toxin into the bloodstream [68], conversely the translocation is helped by AggR-regulated AAF/I adherence to intestinal epithelium enhancing inflammation [19,20,21,22,23,24]. Acid conditions in vitro inhibited S. dublin and EHEC O157:H7 growth in the presence of SCFA, such as acetate [69, 70]. The levels of acetate, propionate and butyrate in the intestinal lumen usually sustains a ratio of approximately 60:20:20 mM, and their abundance is related to the microbiota composition, diet, host genetic features and intestinal trafficking [71, 72]. For instance, during Shigella flexneri infection in vivo, another important human intestinal pathogen, the administration of SCFA, such as acetate, propionate and butyrate, in distinct 60:30:40 mM proportion, resulted in decreased colonization and improved clinical symptoms [73]. The intestinal acetate is mostly produced by bacteria present in the colon, such as Lactobacillus spp., Bifidobacterium spp. and Bacteroides spp. [74], thus, the decline of this SCFA on day 1 p.i. during the C227–11 strain infection (Fig. 3a) is probably related to the sudden drop of these species, leading to an imbalance of its production in this period and reestablishment in the following days (Fig. 2a). On the other hand, the proportion between acetate, propionate and butyrate in each day, remained without significant changes, and could not be directly correlated with microbiota shift in the evaluate period (Figs. 2a, b and 4a). Furthermore, the increase in acetate production on days 2 and 3 p.i. in the C227–11::qseC (Figs. 3b and 4b) are directly correlated with high levels of Lactobacillus spp., Bacteroides spp., and the Firmicutes phylum (Fig. 2c and d), whereas Firmicutes are well known to establish them as the main producer of butyrate [75]. Together with SHIME data, herein the performed in vivo mice infection model for 042 and C227–11 strains with partial disrupted microbiota [44]. These assays have validated that C227–11::qseC infection in vivo also presented lower colonization levels of Lactobacillus spp. after day 1 p.i.. than the WT strain (Fig. 5a). During C227–11 infection the higher levels of Lactobacillus spp. may be correlated with the acetate levels, in the SHIME infection they increase as the progression of infection by day 3 p.i., again specially in the C227–11::qseC strain. Clearly, the QseC seems to be important during the progression of infection, as observed in vivo by the qseC gene expression levels in both EAEC strains (Fig. 5b). Virulence factors such as stx gene expression levels were assayed in vitro during LB growth to evaluate the QseC absence as important factor to attenuate the C227–11 strain (Fig. 5c), like also observed in the C227–11::qseC strain in SHIME® and C57BL/6 infection. The C227–11 has multiple virulence factors probably triggered during different points of the infection in the mice model [42]. However, Shiga toxin important in the host inflammation, may also be employed to interact with the intestinal microbiota, as it is increased in the SHIME® model (Fig. 2e). The microbiota competition and interaction with enteropathogens may be changeling and very fascinating.


The dynamic view of the microbiome, microbial metabolites and infectious process by Shiga toxin-producing C227–11 provided novel insights into the interplay of pathogenic bacteria infection with the microbiota. The QseC kinase sensor seems to modulate the human intestinal microbiota shift during the infectious process by Shiga toxin-producing EAEC C227–11. The SHIME® infection model has proven to be an efficient alternative tool, and correlated with in vivo data, to study pathogen and human microbiota interactions. The QseC sensor kinase of C227–11 strain helped to remodel the gut microbiota, driving distinct abundance in microbiota composition and changed SCFA levels. Finally, our results emphasize the QseC potential as a target for studies in the development of new therapies for EAEC infections.



In this study, we used the EAEC O104:H4 C227–11 strain isolated from elderly patient with hemorrhagic colitis, hospitalized during the outbreak period [29]. The C227–11::qseC strain, gene that encodes the QseC kinase sensor, was previously constructed via pJP5603 suicide vector [42], and all other strains used are listed (Table 1). The qseC mutant strain (::qseC) was complemented with the qseC gene cloned into pBAD33 (SacI/KpnI) as constitutive active vector as previously described [42]. The strains were grown in Luria-Bertani medium (Invitrogen™) with 100 μg/mL of streptomycin, under agitation at 37 °C overnight (16-18 h).

Table 1 Strains used in this study

SHIME® model set up

The Simulator of Human Intestinal Microbial Ecosystem (SHIME®) was used to simulated the human digestion process. The SHIME® reactor is computer-controlled and consists of 5 closed compartments representing the stomach, small intestine, ascending colon, transverse colon and descending colon [46]. The reactor was adapted for this study, where the transverse and descending colon were replaced by the triplicate of the ascending colon (pH 5.6–5.9), aiming to obtain replicates of the experiment for statistical comparison of the data (Fig. 1a), with experimental settings as previously described [49].

Microbiota colonization

The compartments were colonized with feces earlier collected and stored from three healthy volunteers with ages between 18 and 22 years old, according to the procedures [77], adapted to this study [78], and sampling prepared as previously described [49]. All feeding components (Sigma Aldrich, USA) are listed in Table 2.

Table 2 Feed and pancreatic juice composition used in the SHIME®

SHIME® infection

The experimental period in the SHIME® was performed continuously during 5 weeks, as illustrated in Fig. 1b. In the microbiota stabilization period (control), the feed medium (240 mL) and pancreatic juice (60 mL) were inserted into the system as previously described for 14 days [79, 80] (Table 2). A 2 weeks period of stabilization was performed and the first treatment was administered for 72 h. The first infection consisted of 1010 CFU/mL of E. coli C227–11 strain, 240 mL of feed medium and pancreatic juice (60 mL) were added. Between the treatments, a 72 h washout period was performed [49]. After the washout, under similar conditions during the second infection (72 h) started with the 1010 CFU/mL E. coli C227–11::qseC strain in the same conditions, all the experiments were performed in biological triplicates. Selective medium was used to isolate Gram-negative bacilli based on lactose fermentation from the samples of the reactors, when necessary. The EAEC presence and absence was checked in the washout via PCR of exclusive C227–11 gene (Table 3).

Table 3 Oligonucleotides sequences used in this study

Analysis of short-chain fatty acids (SCFA)

The short chain fatty acids were analyzed via gas chromatography as previously described with minor modifications [77]. The samples (n = 3, second week of the colon reactors) were centrifuged (14,000 x g, 5 min) and 2 mL of the supernatant stored for analysis. Analytical curves were constructed from stock solutions of the acids of interest (acetic, propionic and butyric). The samples were filtered through Millex® filters (0.45 μm) into flasks and then injected into an Agilent HP-6890 gas chromatograph equipped with an Agilent model HP-5975 mass-selective detector. A DB-WAX capillary column (60 m × 0.25 mm × 0.25 μm) was used under the following conditions: Injector temperature = 220 °C, column = 35 °C, 2 °C/minute, 38 °C; 10 °C/minute, 75 °C; 35 °C/minute, 120 °C (1 min); 10 °C / min, 170 °C (2 min); 40 °C / minute, 170 °C (2 min), and detector = 250 °C. Helium was used as the carrier gas at a flow rate of 1 mL/minute.

RNA extraction

Samples were collected individually from each ascending colon reactor from day 0 to day 3 p.i. To disrupt the cells and preserve the genetic material, 1 mL of TRIzol® (Ambion) was used for each 100 mg of fecal content. To analyze virulence genes expression, RNA was extracted from late exponential growth phase in LB (O.D.600 1.0). The RNA was purified by RiboPure™ Bacteria Kit (Ambion), according to manufacturer instructions.

Microbiota abundance and gene expression analysis via qRT-PCR

The relative microbiota abundance and relative quantification of gene expression were analyzed via qRT-PCR (Real-Time Quantitative Reverse Transcription PCR), and the reactions was performed using the QuantStudio™ 3 Real-Time PCR Systems (Thermo Fisher Scientific). The reactions were performed in triplicates and final volume of 20 μL, containing Master Mix SYBR®, Multi-scribe® Reverse Transcriptase, RNAse inhibitor (Thermo Fisher Scientific) and 100 ng of RNA. The primers used to analyze phyla, genera, endogenous controls, and individual genes are listed in Table 3. The samples collected independently of each reactor in SHIME® model in the time period listed. As endogenous control, was employed 16S rRNA (Domain Bacteria) for the total of bacteria present in each reactor or rpoA (RNA polymerase subunit A) to gene expression levels. The data were analyzed via Comparative critical threshold (ΔΔCT) [86].

SHIME® washout step controlled via PCR

The PCR (Polymerase Chain Reaction) reactions to verify the absence of O104:H4 C227–11 or C227–11::qseC strains in the washout period, were performed from samples collected independently of each reactor, and lized at 100 °C for 5 min in heat block. This output was employed as DNA template and stx2a set of primers for in the reaction (Table 3). All DNA amplification reactions were performed in the T100™ Thermal Cycler (Bio Rad), with an annealing temperature of 55 °C and extension at 72 °C. The 282 bp PCR product was analyzed on a 1% agarose gel and the images captured on the ChemiDoc MP Imaging System® (Bio-Rad). Conditions for each 50 uL reaction: 35.3 uL of nuclease-free water, 5 uL of buffer (1x), 1uL forward prime (0.2 μM), 1uL of reverse primer (0.2uM), 1.5 μL MgCl2 (1.5 mM), 1uL of DNTP mix (0.2 mM each), 5uL of DNA template from lized cells, 0.2 uL of Invitrogen™ Platinum™ Taq DNA Polymerase (1UI).

Capture ELISA immunoassay

Microtiter plates (C96 Polysorp - NUNC) were incubated at 37 °C for 2 h and then further 4 °C for 16 h with 25 μg/mL of Stx2 polyclonal antibody (pAb) in carbonate-bicarbonate-buffered, pH 9.6. BSA 1% was added as blocking and incubated for 1 h at 37 °C. Material was collected from the reactors and they were incubated for 1 h at 37 °C. Toxin bound to Stx2 pAb were then detected with 5 μg/mL of Stx2 monoclonal antibody followed by anti-mouse IgG peroxidase (Sigma, 15,000) and then with 10 mg/plate of OPD in the presence of hydrogen peroxide. Between incubations the plates were washed three times with PBS-tween 0,05%. Normal microbiota and purified toxin stx2 were used as control. All experiments were carried out in duplicate and results correspond to three independent experiments.

In vivo microbiota assays

The employed mice were acquired from CEMIB/UNICAMP and maintained at our Animal Facility in the Biological Sciences Department at School of Pharmaceutical Sciences/UNESP. The experiment with animals was previously approved by the Animal Ethics Committee (CEUA/FCF/Car 23/2016). Animals were 3- to 5-week-old female C57BL/6 J UNIB mice, weighing between 12 and 15 g. They were pretreated with 20 mg/kg of ampicillin via oral gavage, 24 h before infection, to allow better colonization. Assays were divided into four experimental groups of animals with five (5) mice per group; one group was inoculated with E. coli K-12 DH5a (non-pathogenic) as a negative control. The other three groups were infected, respectively, with C227–11, C227–11::qseC, and EAEC 042 strains. All experiments were repeated at least twice to ensure the results presented here. Strains were cultivated for 16 to 18 h, centrifuged, and resuspended in PBS. Animals were infected with 1010 bacteria via oral gavage. Feces were collected from mice from days 1 to 3 p.i. to be recover, weight loss was monitored and considered for animals with a decrease of at least 5% of total body mass and gene expression was determinated by qRT-PCR as previously described [42].

Statistical analysis

The data were analyzed in the GraphPad Prism 7, and the statistical significance among the groups was determined using the Oneway analysis of variance (ANOVA). P values ≤0.05 were considered statistically significant. The ELISA immunoassay statistical significance analyzes were performed via t-test.

Availability of data and materials

All data generated or analyzed during this study are included in this published article.

Change history


  1. Claesson MJ, Jeffery IB, Conde S, Power SE, O'Connor EM, Cusack S, et al. Gut microbiota composition correlates with diet and health in the elderly. Nature. 2012;488(7410):178–84.

    Article  CAS  PubMed  Google Scholar 

  2. Frick JS, Autenrieth IB. The gut microflora and its variety of roles in health and disease. Curr Top Microbiol Immunol. 2013.

  3. The Human Microbiome Project Consortium. Structure, function and diversity of the healthy human microbiome. Nature. 2012;486(7402):207–14.

    Article  CAS  PubMed Central  Google Scholar 

  4. Neuman H, Debelius JW, Knight R, Koren O. Microbial endocrinology: the interplay between the microbiota and the endocrine system. FEMS Microbiol Rev. 2015;39(4):509–21.

    Article  PubMed  Google Scholar 

  5. Zhang YJ, Li S, Gan RY, Zhou T, Xu DP, Li HB. Impacts of gut Bacteria on human health and diseases. Int J Mol Sci. 2015;16(12):7493–519.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  6. Sharon G, Sampson TR, Geschwind DH, Mazmanian SK. The central nervous system and the gut microbiome. Cell. 2016;167(4):915–32.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  7. Sekirov I, Finlay BB. The role of the intestinal microbiota in enteric infection. J Physiol. 2009;587(Pt 17):4159–67.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  8. McKenney ES, Kendall MM. Microbiota and pathogen 'pas de deux': setting up and breaking down barriers to intestinal infection. Pathog Dis. 2016;74(5); doi:

  9. Buffie CG, Pamer EG. Microbiota-mediated colonization resistance against intestinal pathogens. Nat Rev Immunol. 2013;13(11):790–801.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  10. Byndloss MX, Pernitzsch SR, Baumler AJ. Healthy hosts rule within: ecological forces shaping the gut microbiota. Mucosal Immunol. 2018;11(5):1299–305.

    Article  CAS  PubMed  Google Scholar 

  11. Bergman EN. Energy contributions of volatile fatty acids from the gastrointestinal tract in various species. Physiol Rev. 1990;70(2):567–90.

    Article  CAS  PubMed  Google Scholar 

  12. Macfarlane S, Macfarlane GT. Regulation of short-chain fatty acid production. Proc Nutr Soc. 2003;62(1):67–72.

    Article  CAS  PubMed  Google Scholar 

  13. Tan J, McKenzie C, Potamitis M, Thorburn AN, Mackay CR, Macia L. The role of short-chain fatty acids in health and disease. Adv Immunol. 2014.

  14. Koh A, De Vadder F, Kovatcheva-Datchary P, Backhed F. From dietary Fiber to host physiology: short-Chain fatty acids as key bacterial metabolites. Cell. 2016;165(6):1332–45.

    Article  CAS  PubMed  Google Scholar 

  15. Louis P, Scott KP, Duncan SH, Flint HJ. Understanding the effects of diet on bacterial metabolism in the large intestine. J Appl Microbiol. 2007;102(5):1197–208.

    Article  CAS  PubMed  Google Scholar 

  16. Rivière A, Selak M, Lantin D, Leroy F, De Vuyst L. Bifidobacteria and butyrate-producing Colon Bacteria: importance and strategies for their stimulation in the human gut. Front Microbiol. 2016;7:979.

    Article  PubMed  PubMed Central  Google Scholar 

  17. Kaper JB, Nataro JP, Mobley HL. Pathogenic Escherichia coli. Nat Rev Microbiol. 2004;2(2):123–40.

    Article  CAS  PubMed  Google Scholar 

  18. Hebbelstrup Jensen B, Olsen KE, Struve C, Krogfelt KA, Petersen AM. Epidemiology and clinical manifestations of enteroaggregative Escherichia coli. Clin Microbiol Rev. 2014;27(3):614–30.

    Article  PubMed  PubMed Central  Google Scholar 

  19. Nataro JP, Deng Y, Maneval DR, German AL, Martin WC, Levine MM. Aggregative adherence fimbriae I of enteroaggregative Escherichia coli mediate adherence to HEp-2 cells and hemagglutination of human erythrocytes. Infect Immun. 1992;60(6):2297–304.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  20. Czeczulin JR, Balepur S, Hicks S, Phillips A, Hall R, Kothary MH, et al. Aggregative adherence fimbria II, a second fimbrial antigen mediating aggregative adherence in enteroaggregative Escherichia coli. Infect Immun. 1997;65(10):4135–45.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  21. Boisen N, Struve C, Scheutz F, Krogfelt KA, Nataro JP. New adhesin of enteroaggregative Escherichia coli related to the Afa/Dr/AAF family. Infect Immun. 2008;76(7):3281–92.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  22. Bernier C, Gounon P, Le Bouguénec C. Identification of an aggregative adhesion fimbria (AAF) type III-encoding operon in enteroaggregative Escherichia coli as a sensitive probe for detecting the AAF-encoding operon family. Infect Immun. 2002;70(8):4302–11.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  23. Jonsson R, Struve C, Boisen N, Mateiu RV, Santiago AE, Jenssen H, et al. Novel aggregative adherence fimbria variant of enteroaggregative Escherichia coli. Infect Immun. 2015;83(4):1396–405.

    Article  PubMed  PubMed Central  Google Scholar 

  24. Elias WP Jr, Czeczulin JR, Henderson IR, Trabulsi LR, Nataro JP. Organization of biogenesis genes for aggregative adherence fimbria II defines a virulence gene cluster in enteroaggregative Escherichia coli. J Bacteriol. 1999;181(6):1779–85.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  25. Estrada-Garcia T, Navarro-Garcia F. Enteroaggregative Escherichia coli pathotype: a genetically heterogeneous emerging foodborne enteropathogen. FEMS Immunol Med Microbiol. 2012;66(3):281–98.

    Article  CAS  PubMed  Google Scholar 

  26. Jenkins C. Enteroaggregative Escherichia coli. Curr Top Microbiol Immunol. 2018;416:27–50.

    Article  CAS  PubMed  Google Scholar 

  27. Frank C, Werber D, Cramer JP, Askar M, Faber M, an der Heiden M, et al. Epidemic profile of Shiga-toxin-producing Escherichia coli O104:H4 outbreak in Germany. N Engl J Med. 2011;365(19):1771–80.

    Article  CAS  PubMed  Google Scholar 

  28. Bielaszewska M, Mellmann A, Zhang W, Köck R, Fruth A, Bauwens A, et al. Characterisation of the Escherichia coli strain associated with an outbreak of haemolytic uraemic syndrome in Germany, 2011: a microbiological study. Lancet Infect Dis. 2011;11(9):671–6.

    Article  CAS  PubMed  Google Scholar 

  29. Rasko DA, Webster DR, Sahl JW, Bashir A, Boisen N, Scheutz F, et al. Origins of the E. coli strain causing an outbreak of hemolytic-uremic syndrome in Germany. N Engl J Med. 2011;365(8):709–17.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  30. Dutta PR, Cappello R, Navarro-García F, Nataro JP. Functional comparison of serine protease autotransporters of enterobacteriaceae. Infect Immun. 2002;70(12):7105–13.

    Article  PubMed  PubMed Central  Google Scholar 

  31. Scheutz F, Nielsen EM, Frimodt-Moller J, Boisen N, Morabito S, Tozzoli R, et al. Characteristics of the enteroaggregative Shiga toxin/verotoxin-producing Escherichia coli O104:H4 strain causing the outbreak of haemolytic uraemic syndrome in Germany, May to June 2011. Euro Surveill. 2011;16(24); doi:

  32. Ross BN, Rojas-Lopez M, Cieza RJ, McWilliams BD, Torres AG. The role of long polar fimbriae in Escherichia coli O104:H4 adhesion and colonization. PLoS One. 2015;10(10):e0141845.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  33. Miller MB, Bassler BL. Quorum sensing in bacteria. Annu Rev Microbiol. 2001;55(1):165–99.

    Article  CAS  PubMed  Google Scholar 

  34. Sperandio V, Torres AG, Kaper JB. Quorum sensing Escherichia coli regulators B and C (QseBC): a novel two-component regulatory system involved in the regulation of flagella and motility by quorum sensing in E. coli. Mol Microbiol. 2002;43(3):809–21.

    Article  CAS  PubMed  Google Scholar 

  35. Kendall MM, Sperandio V. What a dinner party! Mechanisms and functions of Interkingdom signaling in host-pathogen associations. MBio. 2016;7(2):e01748–15.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  36. Sperandio V, Torres AG, Jarvis B, Nataro JP, Kaper JB. Bacteria-host communication: the language of hormones. Proc Natl Acad Sci U S A. 2003;100(15):8951–6.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  37. Kim CS, Gatsios A, Cuesta S, Lam YC, Wei Z, Chen H, et al. Characterization of Autoinducer-3 structure and biosynthesis in E. coli. ACS Cent Sci. 2020;6(2):197–206.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  38. Hughes DT, Clarke MB, Yamamoto K, Rasko DA, Sperandio V. The QseC adrenergic signaling cascade in Enterohemorrhagic E. coli (EHEC). PLoS Pathog. 2009;5(8):e1000553.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  39. Rasko DA, Moreira CG, Li de R, Reading NC, Ritchie JM, Waldor MK, et al. Targeting QseC signaling and virulence for antibiotic development. Science. 2008;321(5892):1078–1080, DOI:

  40. Curtis MM, Russell R, Moreira CG, Adebesin AM, Wang C, Williams NS, et al. QseC inhibitors as an antivirulence approach for gram-negative pathogens. MBio. 2014;5(6):e02165.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  41. Ribeiro TRM. Sinalização química e virulência de Escherichia coli O104:H4 (EAEC Stx+). In: Repositório Institucional da Unesp. vol. Dissertação de Mestrado. Araraquara: FCFar/UNESP; 2017.

    Google Scholar 

  42. Machado Ribeiro TR, Cardinali Lustri B, Elias WP, Moreira CG. QseC signaling in the outbreak O104:H4 Escherichia coli strain combines multiple factors during infection. J Bacteriol. 2019;201(17).

  43. Philipson CW, Bassaganya-Riera J, Hontecillas R. Animal models of enteroaggregative Escherichia coli infection. Gut Microbes. 2013;4(4):281–91.

    Article  PubMed  PubMed Central  Google Scholar 

  44. Zangari T, Melton-Celsa AR, Panda A, Boisen N, Smith MA, Tatarov I, et al. Virulence of the Shiga toxin type 2-expressing Escherichia coli O104:H4 German outbreak isolate in two animal models. Infect Immun. 2013;81(5):1562–74.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  45. Molly K, Woestyne MV, Verstraete W. Development of a 5-step multi-chamber reactor as a simulation of the human intestinal microbial ecosystem. Appl Microbiol Biotechnol. 1993;39(2):254–8.

    Article  CAS  PubMed  Google Scholar 

  46. Molly K, Woestyne MV, Smet ID, Verstraete W. Validation of the Simulator of the Human Intestinal Microbial Ecosystem (SHIME) Reactor Using Microorganism-associated Activities. 1994;7(4):191–200.

  47. Ceuppens S, Uyttendaele M, Drieskens K, Heyndrickx M, Rajkovic A, Boon N, et al. Survival and germination of Bacillus cereus spores without outgrowth or enterotoxin production during in vitro simulation of gastrointestinal transit. Appl Environ Microbiol. 2012;78(21):7698–705.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  48. Rooks MG, Garrett WS. Gut microbiota, metabolites and host immunity. Nat Rev Immunol. 2016;16(6):341–52.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  49. Rodrigues V, Duque A, Fino LC, Simabuco FM, Sartoratto A, Cabral L, et al. Modulation of the intestinal microbiota and the metabolites produced by the administration of ice cream and a dietary supplement containing the same probiotics. Br J Nutr. 2020;124(1):1–36.

    Article  Google Scholar 

  50. Roager HM, Licht TR, Poulsen SK, Larsen TM, Bahl MI. Microbial enterotypes, inferred by the prevotella-to-bacteroides ratio, remained stable during a 6-month randomized controlled diet intervention with the new nordic diet. Appl Environ Microbiol. 2014;80(3):1142–9.

    Article  PubMed  PubMed Central  Google Scholar 

  51. LeBlanc JG, Chain F, Martín R, Bermúdez-Humarán LG, Courau S, Langella P. Beneficial effects on host energy metabolism of short-chain fatty acids and vitamins produced by commensal and probiotic bacteria. Microb Cell Factories. 2017;16(1):79.

    Article  CAS  Google Scholar 

  52. Sun Y, O'Riordan MX. Regulation of bacterial pathogenesis by intestinal short-chain fatty acids. Adv Appl Microbiol. 2013.

  53. Walter J, Ley R. The human gut microbiome: ecology and recent evolutionary changes. Annu Rev Microbiol. 2011;65(1):411–29.

    Article  CAS  PubMed  Google Scholar 

  54. Kamada N, Chen GY, Inohara N, Nunez G. Control of pathogens and pathobionts by the gut microbiota. Nat Immunol. 2013;14(7):685–90.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  55. Moreira CG, Weinshenker D, Sperandio V. QseC mediates Salmonella enterica serovar typhimurium virulence in vitro and in vivo. Infect Immun. 2010;78(3):914–26.

    Article  CAS  PubMed  Google Scholar 

  56. Moreira CG, Russell R, Mishra AA, Narayanan S, Ritchie JM, Waldor MK, et al. Bacterial Adrenergic Sensors Regulate Virulence of Enteric Pathogens in the Gut. MBio. 2016;7(3); doi:

  57. Williams KP, Gillespie JJ, Sobral BW, Nordberg EK, Snyder EE, Shallom JM, et al. Phylogeny of gammaproteobacteria. J Bacteriol. 2010;192(9):2305–14.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  58. Cani PD, Amar J, Iglesias MA, Poggi M, Knauf C, Bastelica D, et al. Metabolic endotoxemia initiates obesity and insulin resistance. Diabetes. 2007;56(7):1761–72.

    Article  CAS  PubMed  Google Scholar 

  59. Farhadi A, Banan A, Fields J, Keshavarzian A. Intestinal barrier: an interface between health and disease. J Gastroenterol Hepatol. 2003;18(5):479–97.

    Article  PubMed  Google Scholar 

  60. Drissi F, Buffet S, Raoult D, Merhej V. Common occurrence of antibacterial agents in human intestinal microbiota. Front Microbiol. 2015;6.

  61. Wrzosek L, Miquel S, Noordine ML, Bouet S, Joncquel Chevalier-Curt M, Robert V, et al. Bacteroides thetaiotaomicron and Faecalibacterium prausnitzii influence the production of mucus glycans and the development of goblet cells in the colonic epithelium of a gnotobiotic model rodent. BMC Biol. 2013;11(1):61.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  62. Pickard JM, Zeng MY, Caruso R, Núñez G. Gut microbiota: role in pathogen colonization, immune responses and inflammatory disease. Immunol Rev. 2017;279(1):70–89.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  63. Monteagudo-Mera A, Rastall RA, Gibson GR, Charalampopoulos D, Chatzifragkou A. Adhesion mechanisms mediated by probiotics and prebiotics and their potential impact on human health. Appl Microbiol Biotechnol. 2019;103(16):6463–72.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  64. Levy M, Thaiss CA, Elinav E. Metabolites: messengers between the microbiota and the immune system. Genes Dev. 2016;30(14):1589–97.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  65. Ríos-Covián D, Ruas-Madiedo P, Margolles A, Gueimonde M, de los Reyes-Gavilán CG, Salazar N. Intestinal Short Chain Fatty Acids and their Link with Diet and Human Health. Front Microbiol. 2016. doi:

  66. Havenaar R. Intestinal health functions of colonic microbial metabolites: a review. Benef Microbes. 2011;2(2):103–14.

    Article  CAS  PubMed  Google Scholar 

  67. Tobe T, Nakanishi N, Sugimoto N. Activation of Motility by Sensing Short-Chain Fatty Acids via Two Steps in a Flagellar Gene Regulatory Cascade in Enterohemorrhagic Escherichia coli. Infect Immunity. 2011. doi:

  68. Fukuda S, Toh H, Hase K, Oshima K, Nakanishi Y, Yoshimura K, et al. Bifidobacteria can protect from enteropathogenic infection through production of acetate. Nature. 2011;469(7331):543–7.

    Article  CAS  PubMed  Google Scholar 

  69. El-Gedaily A, Paesold G, Chen CY, Guiney DG, Krause M. Plasmid virulence gene expression induced by short-chain fatty acids in Salmonella Dublin: identification of rpoS-dependent and rpo-S-independent mechanisms. J Bacteriol. 1997;179(4):1409–12.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  70. Shin R, Suzuki M, Morishita Y. Influence of intestinal anaerobes and organic acids on the growth of enterohaemorrhagic Escherichia coli O157:H7. J Med Microbiol. 2002;51(3):201–6.

    Article  CAS  PubMed  Google Scholar 

  71. Chambers ES, Preston T, Frost G, Morrison DJ. Role of gut microbiota-generated short-Chain fatty acids in metabolic and cardiovascular health. Curr Nutr Rep. 2018;7(4):198–206.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  72. Wong JM, de Souza R, Kendall CW, Emam A, Jenkins DJ. Colonic health: fermentation and short chain fatty acids. J Clin Gastroenterol. 2006;40(3):235–43.

    Article  CAS  PubMed  Google Scholar 

  73. Rabbani GH, Albert MJ, Hamidur Rahman AS, Moyenul Isalm M, Nasirul Islam KM, Alam K. Short-chain fatty acids improve clinical, pathologic, and microbiologic features of experimental shigellosis. J Infect Dis. 1999;179(2):390–7.

    Article  CAS  PubMed  Google Scholar 

  74. Fernández J, Redondo-Blanco S, Gutiérrez-del-Río I, Miguélez EM, Villar CJ, Lombó F. Colon microbiota fermentation of dietary prebiotics towards short-chain fatty acids and their roles as anti-inflammatory and antitumour agents: A review. J Funct Foods. 2016;25:511–22.

    Article  CAS  Google Scholar 

  75. Feng W, Ao H, Peng C. Gut microbiota, short-Chain fatty acids, and herbal medicines. Front Pharmacol. 2018;9.

  76. Nataro JP, Baldini MM, Kaper JB, Black RE, Bravo N, Levine MM. Detection of an adherence factor of enteropathogenic Escherichia coli with a DNA probe. J Infect Dis. 1985;152(3):560–5.

    Article  CAS  PubMed  Google Scholar 

  77. Duque ALRF, Monteiro M, Adorno MAT, Sakamoto IK, Sivieri K. An exploratory study on the influence of orange juice on gut microbiota using a dynamic colonic model. Food Res Int. 2016;84:160–9.

    Article  CAS  Google Scholar 

  78. Possemiers S, Marzorati M, Verstraete W, Van de Wiele T. Bacteria and chocolate: a successful combination for probiotic delivery. Int J Food Microbiol. 2010;141(1–2):97–103.

    Article  CAS  PubMed  Google Scholar 

  79. Possemiers S, Verthé K, Uyttendaele S, Verstraete W. PCR-DGGE-based quantification of stability of the microbial community in a simulator of the human intestinal microbial ecosystem. FEMS Microbiol Ecol. 2004;49(3):495–507.

    Article  CAS  PubMed  Google Scholar 

  80. de Wiele TV, Boon N, Possemiers S, Jacobs H, Verstraete W. Prebiotic effects of chicory inulin in the simulator of the human intestinal microbial ecosystem. FEMS Microbiol Ecol. 2004;51(1):143–53.

    Article  CAS  PubMed  Google Scholar 

  81. Guo X, Xia X, Tang R, Zhou J, Zhao H, Wang K. Development of a real-time PCR method for Firmicutes and Bacteroidetes in faeces and its application to quantify intestinal population of obese and lean pigs. Lett Appl Microbiol. 2008;47(5):367–73.

    Article  CAS  PubMed  Google Scholar 

  82. Bacchetti De Gregoris T, Aldred N, Clare AS, Burgess JG. Improvement of phylum- and class-specific primers for real-time PCR quantification of bacterial taxa. J Microbiol Methods. 2011;86(3):351–6.

    Article  CAS  PubMed  Google Scholar 

  83. Fierer N, Jackson JA, Vilgalys R, Jackson RB. Assessment of Soil Microbial Community Structure by Use of Taxon-Specific Quantitative PCR Assays 2005;, 71, 7, 4117, 4120.

    Book  Google Scholar 

  84. Rinttila T, Kassinen A, Malinen E, Krogius L, Palva A. Development of an extensive set of 16S rDNA-targeted primers for quantification of pathogenic and indigenous bacteria in faecal samples by real-time PCR. J Appl Microbiol. 2004;97(6):1166–77.

    Article  CAS  PubMed  Google Scholar 

  85. Brian MJ, Frosolono M, Murray BE, Miranda A, Lopez EL, Gomez HF, et al. Polymerase chain reaction for diagnosis of enterohemorrhagic Escherichia coli infection and hemolytic-uremic syndrome. J Clin Microbiol. 1992;30(7):1801–6.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  86. Walters M, Sperandio V. A autoinducer 3 and epinephrine signaling in the kinetics of locus of enterocyte effacement gene expression in enterohemorrhagic Escherichia coli. Infect Immun. 2006;74(10):5445–55.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

Download references


Not applicable.


We would like to thank our financial support by CAPES to our Graduate Program, CNPq to support our project, and FAPESP Project 2019/03049–7 directly to all funding necessary to reagents, equipments and scientific support.

Author information

Authors and Affiliations



T.R.M.R.: All experiments, design methods and writing; M.K.S.: SHIME®´s experiment, suggestions and writing; M.A.T.A.: SCFA’s analysis and data interpretation; M.A.S.: ELISA assays, analysis, and data interpretation; R.M.F.P.: ELISA assays, analysis, and data interpretation; K.S.: SHIME®´s experiment design, analysis, data interpretation and discussions; C.G.M.: experiments´ design, supervision, funding, and writing. All authors have read and approved the manuscript.

Corresponding author

Correspondence to Cristiano Gallina Moreira.

Ethics declarations

Ethics approval and consent to participate

Not applicable.

Consent for publication

Not applicable.

Competing interests

The authors declare that they have no competing interests.

Additional information

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

The original online version of this article was revised.

Supplementary Information

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit The Creative Commons Public Domain Dedication waiver ( applies to the data made available in this article, unless otherwise stated in a credit line to the data.

Reprints and permissions

About this article

Check for updates. Verify currency and authenticity via CrossMark

Cite this article

Machado Ribeiro, T.R., Salgaço, M.K., Adorno, M.A.T. et al. Human microbiota modulation via QseC sensor kinase mediated in the Escherichia coli O104:H4 outbreak strain infection in microbiome model. BMC Microbiol 21, 163 (2021).

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI: