Review Article | Open Access
C. M. Anjam Khan, "The Dynamic Interactions between Salmonella and the Microbiota, within the Challenging Niche of the Gastrointestinal Tract", International Scholarly Research Notices, vol. 2014, Article ID 846049, 23 pages, 2014. https://doi.org/10.1155/2014/846049
The Dynamic Interactions between Salmonella and the Microbiota, within the Challenging Niche of the Gastrointestinal Tract
Understanding how Salmonella species establish successful infections remains a foremost research priority. This gastrointestinal pathogen not only faces the hostile defenses of the host’s immune system, but also faces fierce competition from the large and diverse community of microbiota for space and nutrients. Salmonella have solved these challenges ingeniously. To jump-start growth, Salmonella steal hydrogen produced by the gastrointestinal microbiota. Type 3 effector proteins are subsequently secreted by Salmonella to trigger potent inflammatory responses, which generate the alternative terminal electron acceptors tetrathionate and nitrate. Salmonella exclusively utilize these electron acceptors for anaerobic respiration, permitting metabolic access to abundant substrates such as ethanolamine to power growth blooms. Chemotaxis and flagella-mediated motility enable the identification of nutritionally beneficial niches. The resulting growth blooms also promote horizontal gene transfer amongst the resident microbes. Within the gastrointestinal tract there are opportunities for chemical signaling between host cells, the microbiota, and Salmonella. Host produced catecholamines and bacterial autoinducers form components of this chemical dialogue leading to dynamic interactions. Thus, Salmonella have developed remarkable strategies to initially shield against host defenses and to transiently compete against the intestinal microbiota leading to successful infections. However, the immunocompetent host is subsequently able to reestablish control and clear the infection.
Salmonella is a major pathogen of the gastrointestinal tract. Our understanding of the cellular and molecular mechanisms by which Salmonella causes disease has been greatly advanced in recent years. In parallel, over the past decade there have been remarkable insights made into our understanding of the human microbiota and its importance in health and disease. Much of this work has largely been descriptive but it has provided essential knowledge on the composition of these communities. For example, the composition of the intestinal microbiota has been determined and provided insightful correlations to health and a variety of disease states, including infections caused by bacterial pathogens. Recently there have been surprising revelations on the dynamic interactions between Salmonella and the intestinal microbiota, as they both compete for essential nutrients and space. The gastrointestinal tract provides a rich and hospitable environment for the microbiota, but the host defends this territory fiercely against invading bacterial pathogens. Remarkably, the hosts frontline defense system is exploited by Salmonella, to inadvertently fuel the “battle of the bugs” and promote a transient growth bloom of Salmonella at the expense of the microbiota and also in detriment to the host. Ultimately, the host is able to successfully reestablish control and clear the infection. This review will provide an introduction on our knowledge and understanding of the biology and pathogenicity of Salmonella and subsequently focus on some of the latest research developments that have provided vivid insights into the dynamic interactions between S. Typhimurium, the resident intestinal microbiota, and the gastrointestinal tract.
2. Salmonella: A Model Enteric Pathogen
The biology and virulence of Salmonella have been intensively studied, providing vivid insights into the mechanisms by which this ingenious pathogen causes disease in mammalian hosts. Key aspects of the virulence mechanisms are discussed below in the context of the biology of Salmonella.
2.1. Salmonella Are Major Global Pathogens
Salmonellae are Gram-negative facultative intracellular bacterial pathogens, which can infect a broad range of animals [1, 2]. Salmonella are rod-shaped bacteria varying in size from about 2 to 3 μm by 0.4 to 0.6 μm, and their rod shape is maintained by an actin-like bacterial cytoskeleton [3, 4]. Salmonella species cause an extensive spectrum of disease in humans from mild gastroenteritis to life-threatening Typhoid fever . Salmonellosis remains a major global health problem causing significant morbidity and mortality. Annually there are 16 million cases of Typhoid fever, 1 billion cases of gastroenteritis, and 3 million deaths across the globe.
Most species can infect a broad range of hosts as is the case for Salmonella enterica serovar Typhimurium (S. Typhimurium), but other serotypes such as S. Typhi, S. Pullorum, and S. Gallinarum are exquisitely host-restricted . Infections in humans lead to acute gastroenteritis, manifested with the clinical symptoms of abdominal pains, nausea, diarrhea, and vomiting. The organisms most frequently associated with this diarrheal disease are S. Typhimurium and S. enterica serovar Enteritidis (S. Enteritidis) and are the leading agents responsible for acute gastroenteritis . In healthy individuals salmonellosis is a self-limiting infection but in the young, the elderly, or the immunosuppressed, Salmonella infections can lead to severe complications and possibly death. In such individuals the infection can spread systemically following breach of the gastrointestinal tract and internalization within phagocytes . Cephalosporins and fluoroquinolones are the preferred antibiotics for treatment of these patients .
Salmonella Species Are Antigenically and Genetically Diverse. The Salmonella genus is divided into two species Salmonella bongori and Salmonella enterica. The species Salmonella enterica is divided further into six subspecies. Based on the presence of distinct surface antigens salmonellae can be divided into over 2500 serovars based on the scheme established by Kauffman and White a century ago . These include flagellar H antigens, somatic lipopolysaccharide O antigens, and virulence (Vi capsular K antigens . From these six subspecies, Salmonella enterica subspecies enterica represents 60% of the 2500 serovars , is most often linked with disease, and is the most diverse. Using whole genome sequence analysis, S. enterica subspecies enterica could be subdivided into two populations, namely, clade A and clade B, reflecting differences in host and tissue tropisms and metabolism .
Achtman and colleagues have also recently used an alternative DNA sequence based approach to investigate by serology . Using multilocus sequence-based typing (MLST) to identify evolutionary relationships, the authors designated the term eBurst groups (eBGs) to signify closely related genetic clusters. Some eBGs matched serovars but many of the clusters identified surprisingly contained multiple serovars. These results clearly suggest that serovar classifications may misdirect epidemiologists and clinicians investigating Salmonella outbreaks and that a DNA-based approach for classification is much needed .
The Escherichia coli (E. coli) and Salmonella enterica (S. enterica) diverged approximately 100 million years ago and their genomes differ by 10%. The S. enterica serovars core genomes differ by less than 1% with each other. They are just under 5 Mb in size and encode for approximately 4,500 genes [11, 13, 14]. The genomes of the enterics have been under intense selective pressures and this is evident in their mosaic genomes. Salmonella have acquired blocks of DNA referred to as Salmonella pathogenicity islands (SPIs) as they encode genes important for virulence . The GC content of this DNA differs from the core genome and the pathogenicity island appears to be integrated into redundant tRNA genes . This suggests they may have been derived from a different bacterial species. Pathogenicity islands provide “quantum leaps” in evolution of bacteria by providing preassembled packages of virulence genes . There are approximately 20 SPIs in Salmonella distributed around the circular chromosome . In addition there is further genetic diversity provided by plasmids, islets, prophages, and phage remnants. Superimposed on top of this variation, Salmonella can undergo genomic rearrangements involving recombination between different rRNA operons and insertion sequences [19, 20].
Chronic Asymptomatic Carriage. In some individuals infection with S. Typhi can lead to chronic asymptomatic carriage . These individuals shed large numbers of bacteria in their feces and can subsequently transmit the pathogen to naïve hosts by contamination of food and water sources. The most famous carrier case is Mary Malone, who was a cook in New York in the early 1900s and became known as “Typhoid Mary” as she transmitted the infection to many others. Livestock have also been identified as carriers, and shedding may play a vital role in epidemics [22, 23].
Emergence and Spread of Multidrug Resistant and Hyper-Virulent Strains. The health and economic burden of this disease is likely to increase due to the rise in multidrug resistant strains and the emergence of new “hyper-virulent” variants . Dougan and colleagues have investigated the emergence in sub-Saharan Africa of a highly invasive nontyphoidal Salmonella (iNTS) strain ST313, a variant of S. Typhimurium . Rather than remaining largely localized around the intestines this variant can now breach the intestinal barrier and colonize humans systemically. Furthermore, the strain appears to have spread from human to human rather than as a zoonosis. Using the power of whole genome sequencing, the investigators observed two distinct lineages of iNTS that appeared approximately 52 to 35 years earlier, correlating in time with the HIV epidemic and treatment of the iNTS with chloramphenicol. Furthermore the strains had accumulated pseudogenes, rather like the invasive and host-restricted S. Typhi responsible for Typhoid fever. These pseudogenes may have promoted the systemic spread of the strains and disease [24, 25]. Thus, immunodeficiency and widespread antibiotic use have been powerful selective forces in the emergence of these highly virulent and drug-resistant strains .
The multidrug resistant S. Typhimurium DT104 has been responsible for global epidemics during the 1990s . DT104 was found to be resistant to ampicillin, chloramphenicol, streptomycin, sulphonamides, and tetracycline and the resistance type is referred to with the acronym ACSSuT . The genes encoding the antibiotic resistance were found to be chromosomally encoded within a locus termed Salmonella genomic island (SGI-1), which is a 43 kb integron . It was popularly believed that this DT104 epidemic was largely a zoonotic infection acquired from eating food products derived from cattle. Using a unique collection of 200 DT104 isolates from a limited geographical area of Scotland, obtained over a 20-year timeframe, Nick Thomson and colleagues began their molecular detective work . Using whole genome sequencing, they investigated the associations between the strains and antibiotic resistance genes . The phylogenetic relationships were established using whole genome sequencing. The results were epidemiologically surprising and provided overwhelming evidence to suggest that contrary to popular belief, the S. Typhimurium DT104 epidemic strains and antibiotic resistance genes were maintained largely independently within human and food animal epidemics, with limited exchange. Antibiotic resistance genes can be transferred horizontally to recipient bacteria as will be discussed in a later section. The authors observed an equally high variability in antibiotic resistance profiles between human and animal isolates. These findings highlight the importance of collecting genotypic data to facilitate our understanding of the ecological basis of epidemics and thus enabling the correct implementation of targeted control measures .
Colonization Beyond Animals. There is an increasing body of evidence to suggest that Salmonella can infect nonanimal hosts and colonize agriculturally important plants . In fact many Salmonella serovars can attach to plants more strongly than the infamous Escherichia coli 0157:H7 . Following attachment, Salmonella can colonize internal plant tissues using virulence genes, which also play an important role in the colonization of animal hosts . Transmission of Salmonella from raw fruit and vegetables to humans is now being increasingly recognized as a major proportion of the reported cases of food poisoning in the United States .
2.2. The Infectious Cycle of Salmonella
The Intestinal Phase. Infections with Salmonella are normally acquired by ingestion of contaminated food and water. Once ingested Salmonella encounter the acidic pH of the stomach which induces an acid tolerance survival response, leading to physiological changes and enabling survival of a small subpopulation . Upon entry into the small intestine, Salmonella are exposed to the destructive effects of the luminal contents including bile salts, enzymes, antimicrobial peptides, and secretory IgA [34, 35]. Salmonella have at least four different infection pathways, namely, via, M-cells, intestinal epithelial cells, CD18-expressing phagocytes, or across a damaged intestinal barrier.
Salmonella travel through the mucous layer to invade intestinal epithelial cells, M-cells, and dendritic cells (DCs). Intestinal epithelial cells are normally nonphagocytic; however, Salmonella have the capacity to invade these cells through a sophisticated machinery termed a type 3 secretion system (T3SS); the genes encoding the T3SS are located on Salmonella pathogenicity island 1 (SPI-1) [36, 37]. Salmonella target specialized M-cells and this initial attachment is promoted by fimbrae . M-cells sit on top of the lymphoid follicles of Peyer’s patches which are normally involved in the pinocytotic sampling of luminal antigens, and this process plays a key role in mucosal immunity. During the process of invasion, Salmonella induce membrane ruffles, which surround the pathogen leading to endocytosis . M-cells transport Salmonella across the epithelial barrier to DCs, which play a key role in innate immune responses.
However, following phagocytosis, Salmonella are able to survive and manipulate the function of the host cell by using effectors of the SPI-2 T3SS (see below), to interfere with, for example, antigen processing and presentation . Salmonella are now able to spread systemically by using DCs as vehicles. Salmonella can also use an alternative strategy to disseminate from the gastrointestinal tract by being taken up by CD18-expressing phagocytes . These phagocytes can transmigrate across tissue barriers and transport Salmonella from the lumen of the gastrointestinal tract to the systemic circulation. Salmonella can also disrupt tight junctions between adjacent epithelial cells, which normally help prevent leakage of water, ions, nutrients, and immune cells from the gastrointestinal tract .
The Systemic Phase. Once Salmonella break across the epithelial cell barrier they are taken up by intestinal macrophages and can initiate systemic disease. In the hostile environment of the phagosome, Salmonella turn on the expression of genes in another horizontally acquired pathogenicity island termed SPI-2 T3SS [43, 44]. The resulting gene products modify the phagosome into a Salmonella containing vacuole (SCV) and remodel the host cell . Collectively these changes lead to a more hospitable environment for the survival and replication of Salmonella. The pathogen can now become disseminated throughout the reticuloendothelial system. In most healthy individuals, Salmonella remain localized to the gastrointestinal tract, which leads to a major migration of neutrophils into intestinal lumen and results in an inflammatory response leading to diarrhea . In most patients the intestinal infection is limited to the small intestine, but in a distinct proportion it involves the colon (colitis). There is a major neutrophil influx into intestinal tissues during human enterocolitis [46, 47]. Stool samples of these enterocolitis patients contain leukocytes dominated by the presence of neutrophils. In otherwise healthy patients, S. Typhimurium infection is self-limiting leading to clearance typically within 14 days and does not require antibiotic treatment .
2.3. Salmonella’s Virulence Machinery Promotes Survival and Transmission
Salmonella enterica encode a variety of virulence factors to promote survival, replication, and transmission of the pathogen into new hosts [49, 50]. Of particular importance to virulence are the type 3 secretion systems (T3SSs) . These secretion systems enable the pathogen to directly inject bacterial effector proteins through a molecular needle-like structure into a host cell to subvert its function. Salmonella harbor two T3SSs encoded on pathogenicity islands SPI-1 and SPI-2. Through the innovative work of Jorge Galan and David Holden and colleagues respectively, vivid insights have been provided into the importance and workings of these two elegant systems [37, 52].
The SPI-1 Type 3 Secretion System Is Important for the Intestinal Phase of Infections. The SPI-1 system appears to be important for the intestinal phase of infection, whereas the SPI-2 system is essential for establishing the systemic phase. These generalized timings for the expression of SPI-1 and SPI-2 genes are now becoming less clearly demarcated [53, 54]. The T3SSs encode for 20 to 30 proteins involved in the assembly of the macromolecular structure termed the needle-complex. The proteins can be functionally classed as being structural, regulatory, chaperones, or effectors of virulence. The T3SS complex basal body spans both the inner and outer bacterial membranes and then continues with a narrower needle complex projecting out from the cell . The SPI-1 T3SS basal body structure is composed of the proteins PrgH, PrgK, and InvG, and the needle itself is composed of polymers of a single subunit protein PrgI. This structure resembles flagella, suggesting an evolutionary connection between these organelles. This is further supported by the observation that T3S structural proteins share sequence identity with flagella proteins . At least three additional proteins are required for the translocation of effector substrates in to host cells, namely, SipB, SipC, and SipD. The assembly of the complex structure takes place through a programmed series of distinct steps, with similarities again to the flagella assembly pathway. Once the structure is fully assembled and energized it is now competent to directly translocate effector substrates in to host cells from the bacterial cytoplasm, without a periplasmic or extracellular phase. There are over 13 effector proteins and a number of which are encoded outside of SPI-1, including SPI-5 and prophages. These proteins include AvrA, SipA, SipB, SipC, SipD, SlrP, SopA, SopB, SopD, SopE, SopE2, SptP, and SspH1, and the list is ever expanding [50, 51, 57]. Indeed SopE is encoded by a lysogenic bacteriophage . As there is no direct evidence to support the notion that effector molecules are transported directly through the needle-complex, a radically alternative view has been suggested based on data with Yersinia . This model, by Hans Wolf-Watz and colleagues, represents a radical shift in our thinking to suggest the needle-complex may in fact play a role in target cell sensing and that effector proteins are secreted through a pore in the host cell membrane . Further, research is needed to validate these secretion models and also it must be noted that they are not mutually exclusive.
Bacterial Mediated Endocytosis. Key SPI-1 T3SS effector proteins are involved in the process of bacterial-mediated endocytosis, and these include SipA, SipC, SopB, SopE, and SopE2. In nonphagocytic cells such as intestinal epithelial cells, these effectors instigate membrane ruffling and engulfment of the bacteria by the “Trigger” mechanism [60, 61]. Koronakis and colleagues have observed that many effectors have acquired multiple functions. For example, SipC is involved in both actin bundling and also actin nucleation [60, 61]. SipA also induces actin bundling and polymerization and formation of the SCV. Furthermore, SipA stimulates neutrophil transmigration and remarkably processes and activates caspase-3 [62, 63].
Receptor-Mediated “Zipper” Entry. A variety of independent experimental approaches have recently provided evidence which challenges the above established “Trigger” mechanism paradigm and suggests that invasion of nonphagocytic host cells by Salmonella can also occur by the “Zipper” mechanism . The Salmonella outer membrane proteins Rck and PagN appear to function as invasins and promote cell invasion. The entry mechanism is independent of T3SSs .
Induction of Potent Inflammatory Responses. Following internalization, the Salmonella effectors induce a potent inflammatory response. The effectors SopB, SopE, and SopE2 activate the small GTPases Cdc42 and Rac-1, stimulating the mitogen-activated protein kinase (MAPK) pathway leading to downstream activation of the transcription factors: activator protein 1 (AP1) and nuclear factor kappa-B (NF-κB) . AP1 and NF-κB elicit the transcription of proinflammatory cytokines such as IL8, which stimulates the transmigration of neutrophils to the intestinal mucosa. SipA alone, as mentioned above, can also trigger signal cascades leading to the transmigration of neutrophils into the intestinal lumen . In addition, SipB has the functionality to activate the caspase-1 inflammasome leading to increases in levels of the proinflammatory cytokines IL-1β and IL-18 . It has also been observed that SopB, SopE, SopE2, and SipA can transiently disrupt epithelial cell tight-junctions and thus disrupt the intestinal barrier, enabling an influx of neutrophils. Through its inositol phosphatase activity SopB stimulates chloride ion secretion and ion fluxes [69, 70]. This leads to the characteristic inflammatory diarrhea, an important feature of gastroenteritis.
The SPI-2 Type 3 Secretion System Is Essential for the Systemic Phase of Infection. Whilst screening for genes essential for systemic growth of Salmonella in mice, Holden and colleagues discovered the SPI-2 T3SS using the innovative technique of signature-tagged mutagenesis [71, 72]. The SPI-2 T3S apparatus has a very similar structure to the SPI-1 T3S needle complex. When Salmonella are taken up or phagocytosed by cells, for example, macrophages, they develop within the Salmonella containing vacuole (SCV). The SCV possesses features of a late endosome including an acidic pH but lacks other characteristic endosome markers and is therefore considered a distinct entity . It has been proposed that the main function of the SPI-2 T3SS is to modify host cell vesicular trafficking, enabling important metabolites to be routed to the SCV and thus providing a safe replication niche. The SPI-2 T3SS genes encoding the secretion machinery are regulated by two-component systems, which include OmpR-EnvZ and also SsrA-B located on SPI-2 itself. The regulatory systems sense the acidic pH and the weak nutritional environment within the SCV. Once a translocon pore is assembled in the SCV membrane, the host cell cytoplasmic pH is sensed, resulting in disassembly of the regulatory complex composed of SpiC, SsaL, and SsaM . This triggers the derepression of delivery of around 30 effector proteins. The effector proteins SifA, SopD2, SseJ, and PipB2 function in the maintenance of the SCV membrane. The effectors SseF and SseG regulate the SCV’s juxtanuclear position near the Golgi apparatus. Effectors also target the host cell cytoskeleton such as SteC, SpvB, SspH2, and SrfH. A number of effectors including SpvC, SspH1, and SseL play key roles in ubiquitin modification and host immune signaling .
3. The Microbiota Live in Intimate Associations with Human Hosts
Complex microbial communities live in intimate association with their human hosts in commensal and also pathogenic interactions. Our understanding of the human microbiota has been completely revolutionized by the pioneering research of Gordon and colleagues [75, 76]. The huge health benefits members of these microbial inhabitants can provide to their hosts are only just beginning to be fully realized and can impact upon diverse conditions as allergies, obesity, diabetes, cancer, and autism. In the sections below we will discuss the benefits the intestinal microbiota can provide against invading bacterial enteropathogens such as Salmonella.
3.1. The Microbiota Is a Large and Diverse Community
A diverse spectrum of microbial communities live in intimate associations with their human hosts and are termed the microbiota . These complex communities contain members from all three domains of life, namely, bacteria, archea, and eukarya. Trillions of bacteria colonize and reside on surfaces within and upon us in mainly a symbiotic relationship. The structure and complexity of these microbial ecosystems vary depending on their location, for example, from the skin to the mouth to the intestine. These microbial communities also provide important ecological benefits to their human hosts based on their locations. In healthy individuals there is a balanced relationship with the microbes, with no resulting disease . The numerical importance of the microbiota can be gauged if we adopt a metrics system of cell numbers, in which case humans equate to being only 10% human and 90% microbe [78, 79]. The diverse population of bacteria that inhabit our bodies is collectively referred to as the bacterial microbiota, and for the purpose of this review we will refer to it simply as the microbiota hereafter. The resident microbiota is in a state of continual flux and undergoes changes from birth through to adulthood of their hosts. They play a key role in maintaining human health by a variety of mechanisms . The human gastrointestinal tract has a large surface area of 200 m2 and the lumen is rich in nutrients [81, 82]. Consequently the gastrointestinal tract provides a very hospitable niche for bacteria. The gastrointestinal tract contains up to 100 trillion bacteria across approximately 1000 species in humans [82, 83]. However, only a small proportion of this microbiota can be cultured and the studies have been reliant on high-throughput sequencing methods to characterize the full range of species present in the microbiota. The resident microbiota colonizes the length and width of the gastrointestinal tract, steadily increasing in numbers from the stomach and duodenum. They vary from as few as 101 bacteria per gram of luminal content in the stomach to 106 bacteria per gram of luminal content in the jejunum and to as many as 1012 bacteria per gram of luminal content in the colon (Figure 1). The colonic bacteria are largely facultative anaerobes and are dominated by the phyla Bacteroidetes and Firmicutes . Actinobacteria, Proteobacteria, Cyanobacteria, Verrucomicrobia, and Fusobacteria are present as a minor fraction of microbiota.
3.2. The Collective Gene Content of the Intestinal Microbiota Is Vast and Provides Huge Benefits for the Host
This enormous community of resident bacteria and their genomes collectively encode the gut “microbiome,” and the microbiome contains more than 100-fold greater number of genes than the human host. The microbiome encodes for biochemical pathways not present in humans which breakdown complex indigestible polysaccharides and proteins. These pathways release and generate essential metabolites including amino acids, vitamins K and B, and short chain fatty acids and are now metabolically available to the benefit of the host. These resident bacteria therefore provide huge paybacks to their hosts. They appear to play key roles promoting the development of the immune system and promoting health. The microbiota can also afford the host protection against invading bacterial pathogens in a process known as “colonization resistance” and will be discussed later .
We Are What We Eat: Diet Shapes the Composition of the Gastrointestinal Microbiota. Diet has a pivotal impact on shaping the composition of the gastrointestinal microbiota . By analyzing detailed nutritional intake in 98 adults with the composition of the microbiota using 16S rDNA sequencing of fecal samples, Wu et al. observed that long-term diet shaped the microbiota enterotypes. For example, intake of animal fat and protein versus carbohydrates correlated with an increased association with Bacteroides or Prevotella species, respectively . Based upon these observations, Turnbaugh and colleagues investigated the short-term impacts of diet changes on the plasticity of the gastrointestinal microbiota using 16S rDNA sequencing . They studied the effects of dietary regimes based on either animal or plant products and found that surprisingly even within a single day, the bacterial community rapidly changed in response to diet . The animal-based diet led to an increase in bacteria tolerant to bile such as Alistipes, Bilophila, and Bacteroides. Furthermore, there were reductions in the numbers of Firmicutes, which metabolize dietary plant polysaccharides including Roseburia, Ruminococcus bromii, and Eubacterium rectale . The bacterial gene expression profiles of specific metabolic modules and pathways also became altered as assessed by RNA sequencing (RNA-seq).
Temporal Stability of the Gastrointestinal Microbiota. There has been a major gap in our knowledge on understanding of how the composition of the microbiota changes throughout the life of an individual. Another landmark study by Jeff Gordon and colleagues has recently addressed this issue by examining fecal microbiota in 37 adults . They determined the composition of the microbiota from these individuals by developing a quantitative low-error 16S ribosomal RNA amplicon sequencing (LEA-seq) method and used this in conjunction with whole-genome sequencing. They observed that 60% of the strains or phylotypes remained stable for 5 years . This stability followed a power-law function and could be statistically extrapolated to potentially remaining stable for decades. In particular Bacteroidetes and Actinobacteria are significantly more stable components than other members of the microbiota. Faith et al. observed that early gastrointestinal tract colonizing microbiota are acquired from our close family members and can potentially mediate their biological effects on health for a significant part of their lives .
Antibiotics Impact on the Composition of the Microbiota. The stability in the composition of the microbiota communities in humans can be modulated by a variety of factors including disease, diet, and medicines. For example, the use of antibiotics in treating infections in humans has a striking effect on the microbiota with a reduction in various taxa and a consequent decrease in bacterial diversity . David Relman and colleagues investigated the effects of the antibiotic ciprofloxacin on the microbiota in three healthy individuals using deep 16S RNA sequencing. Approximately one-third of the bacterial taxa in the gut were reduced in population following antibiotic treatment, and this effect varied amongst individuals. Furthermore, within 4 weeks the composition of the community recovered to preantibiotic treatment levels in all three adults. However, some taxa did not recover even within 6 months . Thus, antibiotic treatments can impact upon the diversity of the microbiota community and as a consequence potentially have longer term impacts on health and disease in hosts.
Postantibiotic Expansion of Enteric Pathogens. The administration of oral antibiotics to humans clearly disrupts the intestinal microbiota and increases the risks associated with acquiring Salmonella and Clostridium difficile infections. A very recent study by Sonnenburg and colleagues provided remarkable mechanistic insights into these observations . These authors used gnotobiotic mice, mono-associated with the Bacteroides thetaiotaomicron and subsequently infected with S. Typhimurium. Following recovery of the pathogen from caecum contents it was subjected to transcriptional profiling. This analysis revealed that genes involved in carbohydrate metabolism were highly upregulated, including three operons involved in the catabolism of sialic acid, fucose, and propanediol, a catabolite of fucose . S. Typhimurium mutants were constructed defective for utilization of sialic acid and fucose and were found to be significantly less competitive than the parent strain in mixed infections in vivo. Compared to germ-free mice, B. thetaiotaomicron colonized mice contained much greater levels of free sialic acid (N-acetylneuraminic acid). B. thetaiotaomicron possesses the enzyme sialidase, which cleaves the terminal sugar from mucosal conjugates. However, if gnotobiotic mice were colonized by a sialidase deficient B. thetaiotaomicron mutant, this significantly reduced pathogen expansion following infection. Sialic acid concentrations were next determined in the ceca of conventional mice following oral antibiotic treatment and revealed a spike in concentration compared to untreated mice. However, S. Typhimurium mutants lacking the ability to catabolize sialic acid were unable to fuel their growth in the mouse intestinal tract following antibiotic treatment. Collectively these data suggest that disruption of the microbiota modulates carbohydrate availability, which is exploited by enteric bacterial pathogens to promote growth. These findings have important therapeutic implications .
3.3. Model Systems for Studying Salmonella Infections and Interactions with the Microbiota
The conventional mouse is the most common model system used to study S. Typhimurium infection and more recently the interactions with the microbiota. Mice can be resistant or genetically susceptible to Salmonella infection. Infection of BALB/c or C57BL/6 mice with S. Typhimurium resembles many aspects of the infection of humans by the host-restricted S. Typhi, leading to Typhoid fever. BALB/c or C57BL/6 mice have a mutation in the gene formerly known as Nramp1 (natural resistance-associated macrophage protein one) and renamed the Slc11a1 gene that leaves them susceptible to systemic infection by S. Typhimurium. The mutation results in a defect in the membrane-bound divalent cation, that is, the Fe2+ anti-porter within the Salmonella containing vacuole in macrophages . The mouse system also offers considerable technical advantages in the availability of immunological tools and transgenic knockout mice.
The mouse model can be adapted to study gastroenteritis by disrupting the normal microbiota using antibiotics . The most popular antibiotic for this purpose is streptomycin. Streptomycin-treated mice when infected with S. Typhimurium develop a disease, which resembles more closely human gastroenteritis, rather than systemic disease. These mice develop an exudative intestinal inflammation with migrated neutrophils in the caecum.
On the other hand, gnotobiotic mice contain defined intestinal microbiota within the gastrointestinal tract and are an attractive model system to study the impact of resident intestinal microbiota on the process of infection . They can range from abiotic germ-free mice, which have no microbiota, to monoassociated or polyassociated mice colonized by known bacterial communities.
The mouse systems have provided excellent models for studying systemic disease. They have yielded a huge wealth of information on the biology and pathogenicity of Salmonella and its interactions with the host and microbiota. However, the mouse model is of very limited use in studying gastroenteritis. Thus, in contrast to mice, natural or experimental infection of calves with S. Typhimurium leads to a localized intestinal disease with many of the hallmarks of a human infection from clinical symptoms to pathology . The calve model offers many practical and technical challenges, however, with only a limited set of genetic and immunological tools, as well as the ethical and financial issues involved.
3.4. The Microbiota Protect the Host from Pathogens by Providing Colonization Resistance
The gastrointestinal tract represents a vast mucosal surface area vulnerable to attack by enteropathogens. The gastrointestinal tract is fortified with a variety of physical and immunological defence barriers. A major protective shield for the gastrointestinal tract and only more recently recognised is the colonising microbiota. This dense population of microbiota is thought to provide both a physical barrier for the attachment of bacterial pathogens to the mucosal surfaces and outcompeting invading pathogens for essential nutrients. This protective mechanism has been termed “colonization resistance” and helps prevent invading bacteria under normal conditions establishing an infection .
The streptomycin-mouse model has provided an important system to study colonization resistance and colitis following S. Typhimurium infection. Oral treatment of mice with the antibiotic streptomycin reduces the microbiota population by approximately 80% and reduces the colonization resistance for window of 24 hours or so. If the mice are now infected with S. Typhimurium this leads now to very efficient colonization of the intestine and especially the cecum and colon where densities as high as 109 colony forming units per gram have been reported . The microbiota population takes around 36 hours to grow back to original levels.
The microbiota also occupies and blocks the binding of pathogens to attachment sites present in the mucous layer. These include carbohydrate groups present within the mucus layer. Many of the specific receptor-ligand interactions that take place still remain to be determined. Bacteroides thetaiotaomicron is an important colonizer of the mucus layer and digests mucin peptides and O-linked glycans as an energy source, resulting in the production of short chain fatty acids (SCFA) such as butyrate [96, 97]. The microbiota is able to produce a nutritional environment not favorable for the growth of bacterial pathogens. For example, the resident microbiota can modify the intestinal composition of carbohydrates and sugars present, which are essential for the growth of pathogens [98, 99]. Furthermore, many microbiota species such as Bifidobacteria and Lactobacillus are able to produce organic acids and SCFAs, which are detrimental to the growth of bacterial pathogens such as S. Typhimurium [100–102]. The microbiota, and in particular members of the Clostridium clusters IV and XIVa, now also known as Ruminococcaceae and Lachnospiraceae, produce the SCFA butyrate as a metabolite [103, 104]. Butyrate is an “antivirulence molecule” which acts as a diffusible signal to downregulate expression of the SPI-1 T3SS invasion genes in Salmonella [103, 105]. In contrast the SCFA formate induces the expression of the SPI-T3SS and invasion . The SCFAs formate and acetate are largely located within the small intestine, whereas butyrate and propionate predominate in the colon .
3.5. Pathogen Clearance: The Microbiota and sIgA Have Complementary Protective Functions
It has been observed that following a Salmonella infection some individuals continue to shed Salmonella in stools once they have become asymptomatic . These asymptomatic excretors are a major transmission risk. To investigate this phenomenon, Baumler and colleagues extended the coverage time of the streptomycin-mouse model to encompass later stages of infection when intestinal mucosal inflammation has begun to decline . As discussed later in this review when the mammalian gastrointestinal tract becomes infected with Salmonella, there is an outgrowth of the pathogen at the expense of the resident microbiota, leading to a substantial reduction in its population size. Following an episode of such an acute infection and decreasing inflammation, pathogen clearance steadily reverses this process by reducing the luminal pathogen load and allowing the microbiota to regrow. This eventually leads to restoration of microbiota composition and numbers to steady-state levels. The mechanistic basis of pathogen clearance remains to be elucidated and conceivably may be multifactorial. For example, it is possible that the microbiota may generate inhibitory molecules or stimulate immunity. The gastrointestinal tract barrier function may also stabilize. An adaptive secretory IgA (sIgA) response is elicited during the later stages of infection and does not appear to play a significant role during this phase of clearance. However, if mice encounter this pathogen again, sIgA specific for S. Typhimurium LPS O-antigen appears to prevent inflammation. Hence, the microbiota and sIgA work in synchrony to protect against pathogens. This is evidently an important area of future research and undoubtedly will have important implications for other pathogens . Nevertheless, host resistance to colonization can be manipulated by successful bacterial pathogens. There have been significant insights into our understanding of the ingenious counter-mechanisms employed by enteropathogens to bridge these lines of defence. These are discussed in later sections.
3.6. Salmonella Can Exploit the Hydrogen Produced by the Resident Microbiota to Jump-Start Initial Growth
In a normal healthy gastrointestinal tract, the resident microbiota generates hydrogen as a central chemical intermediate of metabolism. Wolf-Dietrich Hardt and colleagues have screened for essential genes required during infection in vivo using a transposon mutant bank . Remarkably they identified hyb hydrogenase as playing a key role during the initial growth phases of Salmonella infection, and the findings were validated by a variety of methods including competitive infection experiments. Compelling evidence provided by the authors suggest that during these initial phases of infection, Salmonella can harvest or “steal” the hydrogen produced by the resident microbiota to “jump-start” and fuel their growth bloom .
4. Salmonella Fires Up Mucosal Inflammation in the Gastrointestinal Tract
Enteric pathogens, such as Salmonella, have devised strategies to unlock colonization resistance, compete with microbiota, and successfully infect the host. Vivid insights into the strategies deployed by Salmonella to compete with the resident microbiota have been provided by landmark studies from the laboratories of Andreas Baumler and Wolf-Dietrich Hardt, and colleagues [112, 113]. These studies and their remarkable findings are discussed in the sections below.
4.1. Inflammation Unlocks Colonization Resistance
In the mouse colitis model Wolf-Dietrich Hardt and colleagues observed that the potent inflammatory responses elicited by wild-type S. Typhimurium provided the pathogen with a major competitive growth advantage. This leads to a reduction in the population size of the microbiota and its composition and hence dysbiosis (Figure 2) [114, 115]. Surprisingly an avirulent S. Typhimurium invG, sseD mutant with disruptions in the SPI-1 and SPI-2 T3S systems failed to induce an inflammatory response and the mutant was unable to compete with the microbiota. However, this mutant phenotype could be rescued by inducing inflammation either by coinfection with the wild-type strain or using a transgenic strain of mice IL10−/−, , designed to mimic the inflammatory state in irritable bowel disease. Hence, inflammation is key to surmounting colonization resistance. Thus, inflammation can in some instances benefit the pathogen at the expense of the host and microbiota .
4.2. Mucosal Inflammation Generates Exclusive Terminal Electron Acceptors for Respiration
S. Typhimurium is able to infect intestinal epithelial cells and survive within the hostile environment of professional macrophages. This is possible because Salmonella harbor the SPI-1 and SPI-2 T3SS that enable them to invade and survive within these cell-types. The effector proteins from these secretion systems, for example, SopE, are translocated into host cells to elicit the production of proinflammatory cytokines and potent inflammatory responses . The inflammatory responses are amplified by T-cells located in the intestinal mucosa and release important cytokines.
It has been observed that during S. Typhimurium infections, neutrophils transmigrate in to the intestinal lumen and release reactive oxygen species (ROS) to destroy invading pathogens . The strictly anaerobic Bacteriodetes are dependent on complex polysaccharides and amino acids for fermentation and energy generation . An end product of this fermentation is highly toxic hydrogen sulfide (H2S). This molecule is detoxified by colonic epithelial cells to produce thiosulfate (). However, when thiosulfate becomes exposed to ROS released by neutrophils, it is converted to tetrathionate (; Figure 3) . Andreas Baumler and colleagues have vividly demonstrated that the majority of the microbiota species are unable to biochemically use tetrathionate, but remarkably S. Typhimurium is able to exploit tetrathionate as a terminal electron acceptor in anaerobic respiration (Figure 3) .
Several decades ago a multidrug resistance S. Typhimurium emerged which contained the SopE virulence gene within a prophage. SopE encodes for a SPI-1 T3S effector protein, which stimulates immune signaling pathways and also inflammation of the gastrointestinal tract [116, 119]. The prophage also enhanced the fitness of the strain by unknown mechanisms, and so its role in the mouse colitis model was examined. Baumler and colleagues found that SopE triggers the host to inadvertently generate nitrate, a thermodynamically more efficient terminal electron acceptor than tetrathionate [58, 120]. In the mouse colitis model they observed that there was an increase in mucosal inducible nitric oxide synthetase (iNOS) production following an S. Typhimurium infection. iNOS generates NO which in the presence of ROS forms peroxynitrite (ONOO−). Subsequently, peroxynitrite isomerizes to nitrate (), a terminal electron acceptor that can promote the luminal growth of S. Typhimurium by anaerobic respiration (Figure 3). This nitrate respiration-dependent growth advantage was reduced in iNOS-deficient mice . Interestingly, nitrate also suppresses the expression of bacterial genes involved in the utilization of tetrathionate. This hierarchical control ensures the most energetically efficient electron acceptor is used in the competitive environment of the large intestine. Nitrate thus fuels growth blooms of S. Typhimurium in the inflamed intestine [58, 120].
Thus, the utilization of nitrate or tetrathionate as terminal electron acceptors in respiration is a far more efficient process for energy generation than fermentation. This provides a potentially huge competitive advantage to S. Typhimurium over the resident microbiota and allows the pathogen to access new carbon sources.
4.3. Terminal Electron Acceptors Enable Salmonella to Utilize Unique Substrates for Fermentative Growth Leading to Blooms
The gastrointestinal tractprovides an environment rich in diverse nutrients but the substrates able to support fermentative growth in the anaerobic environment are limited. The situation is exacerbated during inflammatory diarrhea where the rich contents of the gut are rapidly flushed out of the body and no longer available. In the inflamed gastrointestinal tract nutrients may become limited to mucous-derived carbohydrates and the contents of damaged intestinal epithelial cells such as the membrane lipid, phosphatidylcholine. In fact phosphatidylcholine can be readily metabolized to ethanolamine in mammalian intestines. Indeed in calve intestines ethanolamine is readily observed at a concentration of approximately 2 mM . Baumler and colleagues have investigated the ability of S. Typhimurium to utilize ethanolamine . They observed in vitro that ethanolamine could support the growth of S. Typhimurium only in the presence of tetrathionate. To investigate this in vivo, the mouse colitis model was used where mice were treated with streptomycin to disrupt the normal microbiota and then orally infected with a panel of S. Typhimurium mutants including those unable to induce inflammation, for example, SPI-1 and SPI-2 T3S mutants, ethanolamine utilization (eutC), and tetrathionate reductase (ttrA). Through a series of experiments they concluded that in the inflamed gastrointestinal tract, S. Typhimurium is able to use tetrathionate respiration to consume ethanolamine as a nutrient . Ethanolamine cannot be used by the majority of the bacteria in the gut and thus confers S. Typhimurium with a huge growth advantage, which it indeed exploits. The resulting growth bloom in the gastrointestinal tract enhances transmission. Thus, Salmonella has used an ingenious mechanism to trigger inflammation to its benefit but detrimental to the host and competing microbiota.
4.4. Chemotaxis and Flagella-Mediated Motility Enables Salmonella to Identify and Swim to Nutritionally Beneficial Niches
Recent findings using a panel of mutant strains suggest that chemotaxis is important for growth of Salmonella in the inflamed intestinal tract and is dependent on flagella-mediated motility. These attributes may enable S. Typhimurium to migrate to suitable nutritional environments to maximize growth potential. Using chemotaxis, S. Typhimurium senses sugars such as galactose, which is present in high concentrations within the cecal mucosa, and these potential substrates may provide a chemotactic signal. However, the signals are also present in the noninflamed gastrointestinal tract, so what is the nature of the in vivo signal in the inflamed gut? To answer this question, Rivera-Chavez et al constructed a series of mutations in the methyl accepting chemotaxis proteins and the strains examined in the mouse colitis model . The methyl accepting chemotaxis proteins Aer and Tsr were observed to enhance fitness by chemotaxis towards electron acceptors tetrathionate or nitrate, respectively, when these were required to provide a growth advantage in vivo. Thus, the methyl accepting chemotaxis proteins clearly enable the pathogen to “taste” their way to a nutritionally favorable niche and facilitate growth blooms .
4.5. The Gastrointestinal Tract Provides an Environment Conducive to Horizontal Gene Transfer amongst Residents
The entire coding capacity of the microbiota is referred to as the gene pool or “microbiome.” The microbiome can become altered by a variety of factors that affect the abundance of bacterial species. As mentioned previously these factors range from dietary changes, the use of antibiotics, and disease states to the acquisition of new species including pathogens. The resident species can acquire subtle genetic changes by natural point mutations or by the “brute force” of horizontal gene transfer (HGT) . The latter processes enable species to acquire entire blocks of genes, for example, those involved in metabolism, antibiotic resistance, or encoding new virulence factors. Thus, HGT enables the species to evolve at a rapid rate in contrast to the slow accumulation of random point mutations. HGT takes place most efficiently between closely related species, for example, between Enterobacteriaceae. Furthermore, there is strong genomic evidence to suggest that HGT has taken place within the intestinal microbiota . For example, it has been suggested that resistance to bile conferred by a bile salt hydrolase (bsh) present in Bacteroides, Bifidobacterium, Clostridium, Lactobacillus, and Enterococcus may have been acquired by HGT . Under appropriate conditions HGT can also be observed between Enterobacteriaceae and Gram-positives and profoundly even across kingdoms [127–129]. Mechanistically, HGT can take place by transformation, transduction, and conjugation.
DNA Transformation. The uptake of released DNA from “donor” cells in the environment and its stable incorporation and expression within the recipient cells leads to DNA transformation. The ability of recipient strains to take up DNA and recombine it within their genomes is referred to as competence. Transformation in the gastrointestinal tract is expected to be infrequent due to the conditions, which do not favor the survival of free naked DNA. However, it has been suggested that stresses in the gastrointestinal tract may promote competence . Indeed environmental cues such as the presence of chitin have been shown to induce the natural competence of Vibrio cholerae .
Phage Transduction. The DNA of host bacterial cells can be encapsulated by phages and transferred horizontally to recipient bacterial cells, in a process referred to as phage transduction. To promote their own survival within bacteria, phages have acquired additional genes not necessary for their lifecycle but provide a selective advantage for the host bacterium when the phage has integrated into the bacterial genome and is now a prophage. These fitness genes are known as “morons” and make the bacterium more competitive in the intestinal environment. Phages are physically resilient structures, which are expected to survive effectively in the milieu of the gastrointestinal tract. Transduction has clearly been an important mechanism for the transmission of genes as evidenced by genome sequencing where it has been uncovered that many virulence factors in enteropathogens are encoded by prophages. For example, in S. Typhimurium it has been observed that the T3S effector protein SopE is encoded by a prophage . Strikingly there is new evidence to suggest that the acquisition of SopE by HGT stimulates the host to produce the electron acceptor nitrate to fuel a growth bloom of S. Typhimurium in the gastrointestinal tract . Further in the Gram-positive Enterococcus faecalis, a facultative anaerobe and commensal of the human gastrointestinal tract, the acquisition of a composite prophage boosted the fitness of E. faecalis both in vitro and in vivo within the mammalian intestine . These observations suggest that prophages associated with intestinal bacteria have a significant impact in shaping the bacterial communities in the gastrointestinal tract.
Plasmid Conjugation. Direct physical contact between donor and recipient bacteria are required for conjugative transfer of DNA. Conjugative plasmids are transferred to recipient cells through a conjugative pilus encoded by the plasmid. Not surprisingly conjugation efficiency increases with higher cell densities for the donor and recipient cells enabling more conjugative events to take place. As bacterial cell densities are very high within the gut, this niche will provide an environment perfect for promoting conjugative exchange of DNA. These exchanges are facilitated by the optimal growth conditions provided by an influx of nutrients within the gastrointestinal tract and a constant temperature of 37°C.
Norepinephrine Can Modulate HGT. The catecholamine norepinephrine is produced within the gastrointestinal tract, and it has been observed in vitro that norepinephrine, at physiological concentrations, promotes conjugative transfer of a large multidrug resistance plasmid from a clinical strain of S. Typhimurium to an E. coli recipient . Furthermore, this effect appeared to be inhibited by the exposure of the cells to the α-adrenergic receptor antagonist phentolamine. The role of catecholamines in interkingdom signaling will be discussed in a later section.
Inflammation Triggers Bacterial Growth Blooms Which Promotes HGT. A major factor in promoting HGT is inflammation within the gastrointestinal tract leading to very high densities of Enterobacteriaceae . Enterobacteriaceae are normally present in the gastrointestinal tract at low cell densities (<108 cells/mL). Growth blooms in these bacteria can occur due to inflammation caused by invading pathogens such as Salmonella, as discussed already . These blooms are fuelled by the increased availability of high-energy nutrients, which can be used by Enterobacteriaceae or the pathogens but not the resident microbiota. In some elegant studies by Hardt and colleagues it was demonstrated that when mice become infected with S. Typhimurium, the resulting inflammatory responses leads to growth blooms of the pathogen. Furthermore, the resident E. coli are also able to benefit from the products of these inflammatory responses. This results in a rapid elevation in enterobacterial numbers by several orders of magnitude leading to dysbiosis . The increased density of the Enterobacteriaceae facilitates elevated physical contact, resulting in prolific conjugative rates from S. Typhimurium to E. coli of a conjugative plasmid encoding the bacteriocin colicin 1b. Thus, inflammation clearly promotes HGT between closely related bacteria.
Interestingly, Stecher and colleagues have recently demonstrated that within enterobacterial blooms, colicin Ib-mediated killing of competing commensal E. coli confers a distinct growth advantage to S. Typhimurium . The genes encoding colicin Ib (colIb) and its receptor CirA were upregulated in S. Typhimurium and E. coli, respectively, during inflammation . The mosaic genome of Salmonella, containing pathogenicity islands, prophages, transposons, and plasmids, provides evidence for significant levels of HGT during the evolution of this pathogen [11, 18, 136]. Furthermore, in a clinical setting, HGT in the inflamed gut may promote the spread of antibiotic resistance genes between the microbiota and invading pathogens and subsequently selected by antibiotic therapy.
4.6. Host Toll-Like Receptor Sensing of Salmonella Activates the Bacterial Virulence Machinery
The innate immune system plays a vital role in controlling infections once a pathogen has been detected. The system recognizes pathogen-associated molecular patterns (PAMPs) and sets in to play a series of signaling cascades designed to eliminate the pathogen and warn the adaptive immune system of infection [137–139]. PAMPs are recognized by a special family of proteins called toll-like receptors (TLRs). When triggered, TLRs recruit host cell adaptor proteins including MyD88 and TRIF, which activate signaling cascades to promote defense of the host. Each TLR recognizes a particular signature; for example, TLR-4 recognizes lipopolysaccharide from the outer membranes of Gram-negative bacteria, whereas TLR-5 detects bacterial flagellin . TLRs are distributed on the surfaces of many cell-types including macrophages and mucosal epithelial cells.
As discussed earlier Salmonella reside and replicate within host cells such as macrophages by transforming the hostile environment of the phagosome into the Salmonella-containing vacuole. They survive these harsh conditions by turning on the expression of SPI-2 T3SS genes. The T3S effectors enable the pathogen to manipulate the environment of the host cell for its benefit. What are the signals, which turn on expression of the SPI-2 T3SS? Holden and colleagues demonstrated through some elegant studies that expression of SPI-2 T3S is triggered by acidic pH . Using a panel of transgenic TLR knock-out mice, Arpaia et al. have shown that acidification of the phagosome is in fact activated by TLR signaling which rather than protecting the host actually now benefits the pathogen .
4.7. Extinguishing Inflammation in the Gastrointestinal Tract: Hypoarginemia Elevates Susceptibility to Salmonella Infection
The gastrointestinal tract is one of the most metabolically active tissues in humans and has high levels of protein synthesis and cell turnover. Regulation of the gut barrier function is crucial for preventing disease and maintaining good health. The amino acid L-arginine (L-Arg) is not only required for protein synthesis but also appears to be important as a regulator of intestinal function and homeostasis. Indeed the availability of extracellular arginine can impact upon immune defense . This is because arginine is a substrate for inducible nitric oxide synthetase iNOS to generate nitric oxide. Nitric oxide is an effective antimicrobial agent produced by macrophages to combat pathogens but as discussed in this review, nitric oxide can also be exploited by Salmonella through its inflammatory response and used to generate nitrate, which can subsequently be used as a terminal electron acceptor (Figure 3) . Recently it has been observed that malaria-patients develop L-arginine deficiency which reduces intestinal barrier function and makes the patients vulnerable to coinfection with S. Typhimurium . These effects can be compensated by supplementing the diet of patients with arginine, which leads ultimately to improved intestinal barrier function and protection against infection by S. Typhimurium .
5. Salmonella Show Their Metal under Fire
To successfully compete against the resident microbiota within the inflamed gastrointestinal tract, Salmonella must acquire vital nutrients. Some of these nutrients include metals such as iron, zinc, copper and are essential for growth and proliferation [144, 145].
5.1. Salmonella Can Defend against the Effects of Antimicrobial Peptides and Sequester Precious Metals
Within the gastrointestinal tract, pathogens are under attack from host antimicrobial peptides such as lipocalin-2, which are secreted by the intestinal epithelial cells and protect against invading bacteria . Intestinal infections with S. Typhimurium lead to an increase in IL-17 and IL-22 production, which in turn stimulate the intestinal cell production of lipocalin-2, which subsequently accumulates in the lumen. Iron is an essential metal required by bacteria including S. Typhimurium. To scavenge for iron, bacteria can secrete siderophores, such as enterochelin, which bind any available iron in the environment and are subsequently taken up by the bacterial cell. Lipocalin-2 is a 24 kDa glycoprotein which binds to bacterial siderophores, thus starving bacteria of essential iron and preventing growth . However, S. Typhimurium are resistant to the effects of lipocalin-2 as they are able to synthesize an alternative iron binding protein salmochelin. The synthesis and uptake system for salmochelin are encoded by the iroBCDE and iroN genes [148–153]. Salmochelin is a glycosylated derivative of enterochelin, which does not bind lipocalin-2 and is thus resistant to its effects. This resistance provides S. Typhimurium with a significant growth advantage against competing bacteria in the inflamed intestine .
Bacterial pathogens also face a barrage of attack from neutrophils, which have migrated into the intestinal lumen. Approximately 40% of the cytoplasmic nutrient content of neutrophils is composed of a protein named calprotectin . Calprotectin has potent antimicrobial activity against many bacterial pathogens including E. coli and Listeria monocytogenes, due to its ability to bind and sequester essential metals such as zinc and manganese. Raffatellu and colleagues observed that in the presence of S. Typhimurim, neutrophils are induced to release calprotectin . However, S. Typhimurium is able to survive the effects of calpoprotectin by expressing a high affinity zinc transporter (ZnuABC). This transporter enables the pathogen to grab zinc and provides a growth advantage over the competing bacteria in the inflamed environment of the gastrointestinal tract.
5.2. Probiotic Bacteria Pump Iron to Raise Fitness and Outcompete Salmonella
Probiotics are commensal organisms that provide benefits to the host by direct interactions or by competition with pathogens as discussed above in colonization resistance. During an outbreak of shigellosis, a probiotic strain was isolated from a soldier who appeared resistant to an outbreak of diarrhea . The probiotic strain was Escherichia coli Nissle 1917 (serotype O6:K5:H1). The E. coli Nissle strain colonizes the gastrointestinal tract efficiently and has been successfully used as a probiotic for treating intestinal disorders by unknown mechanisms . As acquisition of nutrients such as iron are important for S. Typhimurium, the genome of E. coli Nissle was examined and revealed the presence of multiple iron uptake systems. These include salmochelin, the mixed-type siderophore yersiniabactin, the hydroxamate-type siderophore aerobactin, and the hemin uptake transporter ChuA . Rafettellu and colleagues hypothesized that iron uptake mechanisms are vital for E. coli Nissle probiotic activity. Using the S. Typhimurium colitis mouse models the investigators observed that this nonpathogenic E. coli Nissle was able to outcompete and reduce the size of S. Typhimurium populations during mixed infections. However, when an iron uptake mutant of E. coli Nissle was examined it was found to colonize the intestinal tract but was now unable to dampen down the S. Typhimurim population size . Using the mouse models to examine the impact in further detail, it was observed that iron plays an essential role in promoting the competitiveness of E. coli Nissle in a lipoclain-2 system . The inoculation of E. coli Nissle resulted in a massive reduction in colonization of S. Typhimurium and a general reduction in gastrointestinal inflammation. This study has provided valuable insights in to the mode of action of probiotics, and these organisms could be further developed to provide important benefits to a variety of intestinal diseases.
6. Multidirectional Chemical Signaling within the Gastrointestinal Tract
The gastrointestinal tract contains a highly complex community of host cells, microbiota, together with invading pathogens. These diverse cellular communities provide remarkable opportunities for signaling at multiple levels between the resident microbiota and host cells, together with invading pathogens. Understanding the mechanistic basis of multidirectional chemical signaling will provide important insights into health and disease. These signaling processes may operate at the levels of quorum sensing or interkingdom communication (Figure 4).
6.1. Quorum Sensing with Bacterial Autoinducers
Bacteria synthesize small diffusible signal molecules to count and monitor their population density by a process termed “quorum sensing” [158, 159]. When a critical concentration of this signal molecule is reached, this information is relayed and used to coordinate gene expression within the population and modulate the expression of important phenotypes such as virulence, biofilm formation, and persistence . The bacterially produced signaling molecules are referred to as autoinducers AIs and these molecules are generally very similar in related species . There is now also increasing evidence to suggest that these AIs can also be sensed by species which do not produce the signals themselves, leading to interspecies signaling. These AIs could thus have a major impact on the composition and development of polymicrobial communities in natural settings such as in the environment or a host (Figure 4) [162, 163].
Acyl-homoserine Lactone: An Enteric Signal. Many Gram-negative bacteria, with the notable exceptions of E. coli and Salmonella, quorum sense with N-acyl-homoserine lactone signaling molecule [acyl-HSL] also known as autoinducer-1 [AI-1] . LuxI synthesizes the QS signal molecule, which is subsequently detected by the cognate sensor and transcriptional regulator LuxR. Acyl-HSL can vary in their acyl side chain length from 4 to 18 carbons. Although neither E. coli nor Salmonella synthesize acyl-HSL, they do possess a LuxR orthologue known as SdiA. Consequently they can sense acyl-HSLs produced by other bacterial species in a process aptly termed “eavesdropping” . These enterics can infect the intestinal tracts of humans and animals and it maybe that Salmonella and E. coli are able to detect acyl-HSLs produced by members of the intestinal microbiota and use these signals as an environmental cue to regulate gene expression. Barring physical degradation of the acyl-HSLs, there appears to be no chemical or biological evidence to support this notion. However, Ahmer and colleagues used a clever genetic screen, a recombination-based in vivo expression technology (RIVET) reporter system, in which SdiA dependent detection of acyl-HSLs would result in a permanent deletion of a tetracycline resistance gene during the passage of Salmonella through a host [164–167]. The Salmonella infection reporter screen did not detect any acyl-HSL during infections of a number of animals ranging from mice to chickens to cows. However, the reporter was found to become active in turtles and also in mice, which had been infected with the pathogen Yersinia enterocolitica . Thus, it appears that the intestinal microbiota does not appear to produce detectable levels of acyl-HSLs, but some intestinal pathogens can generate acyl-HSLs enabling S. Typhimurium to eavesdrop on these quorum sensing pathogens when coinfecting the host. The competitive advantages of acyl-HSL eavesdropping for Salmonella remain to be elucidated.
The “Universal” Signal Autoinducer 2. The majority of both Gram-negative and Gram-positive bacteria possess the enzyme LuxS that is an AI-2 synthase or S-ribosyl homocysteine lyase, including members of the intestinal microbiota such as Bacteroides species. AI-2 is believed to be a QS signaling molecule, which has been referred to as a universal signaling molecule due to the widespread distribution of luxS . In the well-studied Vibrio harveyi system, AI-2 is a furanosyl borate diester. In contrast to S. Typhimurium, AI-2 has the identity of (2R,4S)-2-methyl-2,3,3,4-tetrahydroxytetrahydrofuran (R-THMF) and lacks boron . The role of AI-2 as a true QS signaling molecule remains to be unequivocally demonstrated in most cases [163, 169, 170]. In bacterial species studied to date AI-2/luxS appears to regulate expression of genes involved in virulence, biofilm formation, motility, and carbohydrate metabolism. In S. Typhimurium, AI-2 affects the expression of the AI-2 uptake system the Lsr operon [171–173]. However, LuxS plays an important metabolic role in the activated methyl cycle, and its role in metabolism could have an impact on the observed phenotypes. This is supported by the following observations. In S. Typhimurium it has been demonstrated that a luxS gene deletion mutant modulates flagellar phase variation independent of AI-2 leading to expression of phase-1 flagellin subunits [174, 175]. Complementation studies revealed this phenotype appeared to be dependent on the small RNA micA located immediately upstream to the luxS coding sequence rather than the luxS gene product itself [174, 176]. The same observation is true for Salmonella biofilm formation . Furthermore, in Streptococcus sanguinis, complementation of the active methyl cycle with the S-adenosylhomocysteine hydrolase (SahH) gene restores biofilm formation independently of AI-2 and luxS . The picture is also complicated as the luxS deletion mutant also has pleiotropic effects on S. Typhimurium gene expression . As a consequence of the pleiotropic effects on bacterial metabolism, AI-2 has also been indirectly implicated in the production of another autoinducer (AI-3) in E. coli and also Salmonella [179, 180].
It has recently been demonstrated that Bacteroides species can produce AI-2 like molecules , and heterologous expression of Bacteroides luxS orthologues can complement AI-2 production in E. coli . As members of the intestinal microbiota produce AI-2, it is not inconceivable that members of these dense communities exploit LuxS-based signaling to modulate gene expression and community phenotypes.
Commensal Bacterial Indole Signals Diminishes the Pathogenicity of Salmonella. There is increasing evidence to suggest that indole signaling is used by bacteria within the gastrointestinal tract for communication . In commensal E. coli the environmental conditions of the intestine induce the expression of tryptophanase (tnaA), the enzyme that generates indole. Indole concentrations in the mammalian intestine can vary from 250 μM to 1 mM .
Indole is produced by E. coli in stationary phase cells and appears to regulate biofilm formation, acid resistance, and the locus for enterocyte effacement in pathogenic E. coli . Indole also elevates the expression of multidrug exporters and has an impact on population based antibiotic resistance in E. coli. Indole signaling clearly affects membrane and oxidative stress response. Following on from this it has been demonstrated that indole induces the formation of persisters, where a fraction of the isogenic bacteria in a population “tolerate” antibiotics. Persister formation was monitored by Collins and colleagues by the novel use of microfluidics, combined with fluorescence microscopy and DNA microarray screens . They identified stress response pathways, including OxyR and phage stress response (Psp), which were essential for persister formation. Thus, E. coli can use a “bet-hedging” strategy when nutrients are limited by producing a heterogeneous population of bacteria to improve their chances of survival .
Curiously S. Typhimurium is unable to produce indole as it does not have the tryptophanase enzyme. However, indole has been observed to induce the expression of the S. Typhimurium acrAB-tolC multidrug efflux system and this phenotype is dependent upon the regulator RamA. Intriguingly using DNA microarrays the authors observed that indole downregulated the expression of the SPI-1 T3SS genes and also genes involved in motility . These changes were directly manifested phenotypically by a reduction in invasiveness and motility. These phenotypes as discussed elsewhere in this review are clearly important for eliciting an inflammatory response in the host and benefits Salmonella competitively at a nutritional level over competing microbiota, including commensal E. coli, leading to growth blooms. Thus, this may be a mechanism designed by members of the microbiota to dampen the competitiveness of S. Typhimurium and reduce the growth blooms. This suggests that indole could potentially be used therapeutically to control infections against bacterial pathogens such as S. Typhimurium.
Intestinal Cells Can Intercept Bacterially Produced Indole to Fortify Host Defense Barriers. From the previous sections there is convincing evidence to suggest interkingdom communication can take place by bacteria eavesdropping on host signaling molecules such as hormones (Figure 4). Bacteria also exploit indole as a signaling molecule as discussed. The physiological impact of bacterially produced indole on host intestinal cells was investigated by Jayaraman and colleagues . They observed changes in gene expression in the human enterocyte HCT-8 cell line when exposed to physiological concentrations of indole using DNA microarrays and phenotypic screens. They observed that indole increased expression of anti-inflammatory genes and the downregulation of some proinflammatory genes. Furthermore, genes involved in enhancing the mucosal barrier such as actin-cytoskeleton and tight-junction proteins were elevated, with increases in mucin gene expression and production. This led to an increase in the transepithelial cell resistance of the HCT-8 cells suggesting the mucosal barrier had been fortified . This reduces the ability for enteric pathogens to traverse the intestinal epithelial cell barrier by increasing its integrity and resistance to invasion. The findings of this research also suggest that indole could be used to treat inflammatory intestinal bowel disorders such as Crohn’s disease by enhancing the epithelial cell barrier and dampening inflammation.
6.2. Interkingdom Signaling within the Gastrointestinal Tract
Catecholamines such epinephrine and norepinephrine are key players in mediating acute host stress. Half of the norepinephrine in the human body is produced by the neuroendocrine system within the gastrointestinal tract. Through the original investigations by Lyte and colleagues it has now become established that bacteria can sense and respond to host produced signaling molecules such as norepinephrine and epinephrine [188, 189]. These findings have given birth to new field, aptly coined by Lyte as “microbial endocrinology” (Figure 4) .
Microbiota Play a Pivotal Role in the Production of Catecholamines. Catecholamines are produced by the neuroendocrine system within the gastrointestinal tract and it was believed the resident commensals played no role in this process. To determine whether the intestinal microbiota had an impact on catecholamine production, Asano and colleagues have overcome some major technical challenges and determined the physical levels of catecholamines norepinephrine and dopamine using HPLC . Using pathogen-free mice, germ-free mice, and gnotobiotic mice, the authors determined the catecholamine levels in the gastrointestinal tract of these mice. Their studies revealed that pathogen-free mice had elevated levels of catecholamines when compared to germ-free mice, which had no intestinal microbiota. However, the introduction of either: specific pathogen-free mice fecal bacteria, E. coli, or Clostridium species into germ-free mice resulted in a remarkable increase in the levels of biologically active dopamine and norepinephrine. Furthermore, the authors went on to observe that an E. coli mutant unable to produce β-glucuronidase was no longer able to raise the levels of free biologically active catecholamines, thus suggesting the bacterial enzyme plays a key role in the hormone maturation process . This powerful comparative approach has vividly revealed that the resident gut microbiota and the bacterial enzyme β-glucuronidase have pivotal roles in the production of biologically active catecholamines in the gastrointestinal tract of the host.
Catecholamines in the Gastrointestinal Tract Regulate the Virulence of Salmonella. The gastrointestinal pathogen enterohemorrhagic Escherichia coli (EHEC) harbors a pathogenicity island named the locus of enterocyte effacement (LEE). A relatively new bacterial autoinducer has been reported, AI-3, which stimulates the expression of the LEE virulence operon in EHEC colitis. The sensing of AI-3 and signaling takes place through the two-component signal transduction systems QseBC and QseEF. These two-component systems regulate virulence by modulating the expression of the LEE locus [192, 193]. Astonishingly the catecholamines epinephrine and norepinephrine can imitate the same biological effects of AI-3 [192, 193]. Furthermore, α- and β-adrenergic receptor antagonists can block the signaling.
These hormones also have an impact on the virulence of Salmonella [163, 174, 194, 195]. Lipopolysaccharide is an important molecule in the outer membranes of Gram-negative bacteria and is subject to modification to help adapt the bacterium to survive in different environments. For example, the structure of LPS can be modified by the pmr operon in Salmonella to adapt to different environments; for example, in the gastrointestinal tract Paneth cells are an important source of antimicrobial peptides. The pmr operon confers resistance to antimicrobial peptides such as polymyxin B. If Salmonella are exposed to epinephrine and subsequently challenged with polymyxin B, they become more sensitive to the effects of this cationic antimicrobial peptide . However, the effect is fully reversible with the addition of propranolol, a β-adrenergic blocker . The phenotype was independent of QseC, and through genetic screens the BasSR two-component signal transduction system was identified as being essential for this observation. The LPS modifying enzymes PmrF and PagL are down-regulated by epinephrine leading to an altered LPS chemotype. These modifications in the structural configuration of LPS can increase the sensitivity of the pathogen to antimicrobial peptides, and also subdue the host inflammatory responses as the modified LPS now reduces activation of the TLR-4 receptors .
The exclusively human pathogen S. Typhi can sense and respond to catecholamine hormones and release the toxin HlyE in outer membrane vesicles . The signaling cascades involve the two-component system CpxAR, with increased expression of the sRNA micA and the RNA chaperone Hfq. This complex is believed to block the translation of the ompA mRNA leading to reduced amounts of OmpA in the outer membrane. This facilitates the release of outer membrane vesicles containing HlyE [163, 194, 198]. From the above examples, adrenergic signaling is clearly a double-edged sword, which can provide benefits to the pathogen but also on occasions to the host.
Fucose Sensing and Intestinal Colonization. B. thetaiotaomicron is believed to possess fucosidases, which cleave fucose from glycans such as mucin [199, 200]. Very recently it has been reported that fucose can be sensed by the gastrointestinal pathogen EHEC to regulate the expression of virulence genes located within the LEE locus . Expression of genes in this locus is activated by the bacterial signal AI-3 and host catecholamines as described above. Sensing of fucose is mediated by a two-component system FusKR located on the pathogenicity island OI-20 and appears to downregulate expression of the LEE locus . Furthermore, QseBC and QseEF repress the expression of FusKR. These findings suggest that EHEC is able to sense fucose produced by the intestinal mucosa and subsequently modulate the expression of virulence genes . The rationale behind this reciprocal regulation is puzzling, as the catecholamines and AI-3 signal would be expected to be in very similar locations as the fucose signal. Clearly further research is required to definitively answer this question and also whether other enteric pathogens such as S. Typhimurium are able to sense and respond to fucose to modulate virulence gene expression.
7. Concluding Remarks and Future Perspectives
Salmonella possess an armory of virulence factors to enable efficacious infection of their hosts. Many of these virulence factors protect the pathogen against host defenses and enable Salmonella to invade and colonize mammalian tissues. Central to these processes are the SPI-1 and SPI-2 T3SSs, which have been acquired by ancestor strains through horizontal gene transfer. There are a wealth of interactions between Salmonella, the microbiota, and the gastrointestinal tract. In contrast to S. Typhi, it is believed that S. Typhimurium deliberately engages the host inflammatory response through the SPI-1 and SPI-2 T3SSs. The inflamed intestine provides S. Typhimurium with competitive growth advantages over the resident microbiota, by enabling the generation of unique electron acceptors and the subsequent utilization of new substrates by the pathogen. S. Typhimurium can thus overcome “nutritional immunity” by strategically modifying its immediate environment enabling them to efficaciously outcompete the resident microbiota. It is essential to determine the contents of the inflamed intestine by metabolomics to facilitate the identification of potential substrates and understand how Salmonella manipulate the nutritional environment of the gastrointestinal tract. Anaerobic respiration could also provide a therapeutic target to control infections, and this needs to be explored.
The intestine provides a very rich and dense ecosystem enabling complex signaling between the host gastrointestinal cells, the resident microbiota, and invading bacterial pathogens. Bacteria generate a plethora of signaling molecules and through their intimate interactions with mammalian hosts have acquired the abilities to intercept host signals. Metabolomic approaches to comprehensively analyze intestinal contents may facilitate the identification of such signaling molecules. Understanding these elaborate signaling cascades will be central to gaining a full understanding of the processes required for maintaining good health and preventing disease.
The present research at understanding the interactions between the host cells, microbiota, and bacterial pathogens has been limited to model organisms. These models have proved very valuable but have limitations. Future research should aim to examine these interactions directly within the natural hosts for Salmonella, from livestock to humans. The rapid technological advances taking place in rRNA sequencing as well as whole-genome sequencing will facilitate these systems biology based approaches. Investigators are now shifting their objectives from collecting a descriptive analysis of the microbiota community composition and their associations with health and disease to delivering more fundamental mechanistic insights into the dynamic interactions between the host, resident microbiota, and invading pathogens.
Conflict of Interests
The author declares that there is no conflict of interests regarding the publication of this paper.
The research in the laboratory of the author was supported by grants from the Medical Research Council UK and also the Newcastle upon Tyne Hospitals NHS Charity. The author expresses their sincere apologies to colleagues whose important research has not been cited or discussed due to space limitations and brevity. The author thanks David Bulmer and Paul Dean for helpful comments and the author is also grateful to the three anonymous reviewers for their valuable observations and suggestions. Finally, this spotlight review article is dedicated to my inspirational parents Yasmin and Aslam Khan.
- H. Ochman and E. A. Groisman, “The origin and evolution of species differences in Escherichia coli and Salmonella typhimurium,” EXS, vol. 69, pp. 479–493, 1994.
- A. J. Bäumler, R. M. Tsolis, T. A. Ficht, and L. G. Adams, “Evolution of host adaptation in Salmonella enterica,” Infection and Immunity, vol. 66, no. 10, pp. 4579–4587, 1998.
- D. M. Bulmer, L. Kharraz, A. J. Grant et al., “The bacterial cytoskeleton modulates motility, type 3 secretion, and colonization in Salmonella,” PLoS Pathogens, vol. 8, no. 1, Article ID e1002500, 2012.
- A. C. Doble, D. M. Bulmer, L. Kharraz, M. H. Karavolos, and C. M. A. Khan, “The function of the bacterial cytoskeleton in Salmonella pathogenesis,” Virulence, vol. 3, no. 5, pp. 446–449, 2012.
- J. Fierer and D. G. Guiney, “Diverse virulence traits underlying different clinical outcomes of Salmonella infection,” Journal of Clinical Investigation, vol. 107, no. 7, pp. 775–780, 2001.
- S. Spanò and J. E. Galán, “A Rab32-dependent pathway contributes to Salmonella typhi host restriction,” Science, vol. 338, no. 6109, pp. 960–963, 2012.
- W. Rabsch, H. Tschäpe, and A. J. Bäumler, “Non-typhoidal salmonellosis: emerging problems,” Microbes and Infection, vol. 3, no. 3, pp. 237–247, 2001.
- N. A. Feasey, G. Dougan, R. A. Kingsley, R. S. Heyderman, and M. A. Gordon, “Invasive non-typhoidal Salmonella disease: an emerging and neglected tropical disease in Africa,” The Lancet, vol. 379, no. 9835, pp. 2489–2499, 2012.
- P. Butaye, G. B. Michael, S. Schwarz, T. J. Barrett, A. Brisabois, and D. G. White, “The clonal spread of multidrug-resistant non-typhi Salmonella serotypes,” Microbes and Infection, vol. 8, no. 7, pp. 1891–1897, 2006.
- M. Y. Popoff, J. Bockemühl, and L. L. Gheesling, “Supplement 2002 (no. 46) to the Kauffmann-White scheme,” Research in Microbiology, vol. 155, no. 7, pp. 568–570, 2004.
- H. C. den Bakker, A. I. Moreno Switt, G. Govoni et al., “Genome sequencing reveals diversification of virulence factor content and possible host adaptation in distinct subpopulations of Salmonella enterica,” BMC Genomics, vol. 12, article 245, 2011.
- M. Achtman, J. Wain, F. X. Weill et al., “Multilocus sequence typing as a replacement for serotyping in Salmonella enterica,” PLoS Pathogens, vol. 8, no. 6, Article ID e1002776, 2012.
- M. McClelland, K. E. Sanderson, J. Spieth et al., “Complete genome sequence of Salmonella enterica serovar Typhimurium LT2,” Nature, vol. 413, no. 6858, pp. 852–856, 2001.
- J. Parkhill, G. Dougan, K. D. James et al., “Complete genome sequence of a multiple drug resistant Salmonella enterica serovar Typhi CT18,” Nature, vol. 413, no. 6858, pp. 848–852, 2001.
- M. Hensel, “Evolution of pathogenicity islands of Salmonella enterica,” International Journal of Medical Microbiology, vol. 294, no. 2-3, pp. 95–102, 2004.
- J. Hacker and J. B. Kaper, “Pathogenicity islands and the evolution of microbes,” Annual Review of Microbiology, vol. 54, pp. 641–679, 2000.
- E. A. Groisman and H. Ochman, “Pathogenicity islands: bacterial evolution in quantum leaps,” Cell, vol. 87, no. 5, pp. 791–794, 1996.
- S. C. Sabbagh, C. G. Forest, C. Lepage, J. M. Leclerc, and F. Daigle, “So similar, yet so different: uncovering distinctive features in the genomes of Salmonella enterica serovars Typhimurium and Typhi,” FEMS Microbiology Letters, vol. 305, no. 1, pp. 1–13, 2010.
- X. Didelot, R. Bowden, T. Street et al., “Recombination and population structure in Salmonella enterica,” PLoS Genetics, vol. 7, no. 7, Article ID e1002191, 2011.
- H. K. de Jong, C. M. Parry, T. van der Poll, and W. J. Wiersinga, “Host-Pathogen Interaction in Invasive Salmonellosis,” PLoS Pathogens, vol. 8, no. 10, Article ID e1002933, 2012.
- M. M. Levine, R. E. Black, and C. Lanata, “Precise estimation of the number of chronic carriers of Salmonella typhi in Santiago, Chile, an endemic area,” Journal of Infectious Diseases, vol. 146, no. 6, pp. 724–726, 1982.
- S. Gopinath, S. Carden, and D. Monack, “Shedding light on Salmonella carriers,” Trends in Microbiology, vol. 20, no. 7, pp. 320–327, 2012.
- D. M. Monack, “Salmonella persistence and transmission strategies,” Current Opinion in Microbiology, vol. 15, no. 1, pp. 100–107, 2012.
- C. K. Okoro, R. A. Kingsley, T. R. Connor et al., “Intracontinental spread of human invasive Salmonella Typhimurium pathovariants in sub-Saharan Africa,” Nature Genetics, vol. 44, no. 11, pp. 1215–1221, 2012.
- S. Baker and G. Dougan, “The genome of Salmonella enterica serovar typhi,” Clinical Infectious Diseases, vol. 45, supplement 1, pp. S29–S33, 2007.
- E. J. Threlfall, “Epidemic Salmonella typhimurium DT 104—a truly international multiresistant clone,” Journal of Antimicrobial Chemotherapy, vol. 46, no. 1, pp. 7–10, 2000.
- D. A. Boyd, X. Shi, Q. H. Hu et al., “Salmonella genomic island 1 (SGI1), variant SGI1-I, and new variant SGI1-O in Proteus mirabilis clinical and food isolates from China,” Antimicrobial Agents and Chemotherapy, vol. 52, no. 1, pp. 340–344, 2008.
- A. E. Mather, S. W. Reid, D. J. Maskell et al., “Distinguishable epidemics of multidrug-resistant Salmonella Typhimurium DT104 in different hosts,” Science, vol. 341, no. 6153, pp. 1514–1517, 2013.
- A. Schikora, A. V. Garcia, and H. Hirt, “Plants as alternative hosts for Salmonella,” Trends in Plant Science, vol. 17, no. 5, pp. 245–249, 2012.
- J. D. Barak, L. C. Whitehand, and A. O. Charkowski, “Differences in attachment of Salmonella enterica serovars and Escherichia coli O157:H7 to alfalfa sprouts,” Applied and Environmental Microbiology, vol. 68, no. 10, pp. 4758–4763, 2002.
- J. T. Noel, N. Arrach, A. Alagely, M. Mcclelland, and M. Teplitski, “Specific responses of Salmonella enterica to tomato varieties and fruit ripeness identified by in Vivo expression technology,” PLoS ONE, vol. 5, no. 8, Article ID e12406, 2010.
- N. Holden, L. Pritchard, and I. Toth, “Colonization outwith the colon: Plants as an alternative environmental reservoir for human pathogenic enterobacteria: review article,” FEMS Microbiology Reviews, vol. 33, no. 4, pp. 689–703, 2009.
- F. Garcia-Del Portillo, J. W. Foster, and B. B. Finlay, “Role of acid tolerance response genes in Salmonella typhimurium virulence,” Infection and Immunity, vol. 61, no. 10, pp. 4489–4492, 1993.
- A. M. Prouty, I. E. Brodsky, S. Falkow, and J. S. Gunn, “Bile-salt-mediated induction of antimicrobial and bile resistance in Salmonella typhimurium,” Microbiology, vol. 150, no. 4, pp. 775–783, 2004.
- P. Michetti, M. J. Mahan, J. M. Slauch, J. J. Mekalanos, and M. R. Neutra, “Monoclonal secretory immunoglobulin A protects mice against oral challenge with the invasive pathogen Salmonella typhimurium,” Infection and Immunity, vol. 60, no. 5, pp. 1786–1792, 1992.
- J. E. Galan and R. Curtiss III, “Cloning and molecular characterization of genes whose products allow Salmonella typhimurium to penetrate tissue culture cells,” Proceedings of the National Academy of Sciences of the United States of America, vol. 86, no. 16, pp. 6383–6387, 1989.
- J. E. Galán, “Salmonella interactions with host cells: type III secretion at work,” Annual Review of Cell and Developmental Biology, vol. 17, pp. 53–86, 2001.
- A. J. Bäumler, R. M. Tsolis, and F. Heffron, “Contribution of fimbrial operons to attachment to and invasion of epithelial cell lines by Salmonella typhimurium,” Infection and Immunity, vol. 64, no. 5, pp. 1862–1865, 1996.
- B. D. Jones, N. Ghori, and S. Falkow, “Salmonella typhimurium initiates murine infection by penetrating and destroying the specialized epithelial M cells of the Peyer's patches,” Journal of Experimental Medicine, vol. 180, no. 1, pp. 15–23, 1994.
- A. Leoni Swart and M. Hensel, “Interactions of Salmonella enterica with dendritic cells,” Virulence, vol. 3, no. 7, pp. 660–667, 2012.
- A. Vazquez-Terres, J. Jones-Carson, A. J. Bäumler et al., “Extraintestinal dissemination of Salmonella by CD18-expressing phagocytes,” Nature, vol. 401, no. 6755, pp. 804–808, 1999.
- M. A. Jepson, C. B. Collares-Buzato, M. A. Clark, B. H. Hirst, and N. L. Simmons, “Rapid disruption of epithelial barrier function by Salmonella typhimurium is associated with structural modification of intercellular junctions,” Infection and Immunity, vol. 63, no. 1, pp. 356–359, 1995.
- J. E. Shea, M. Hensel, C. Gleeson, and D. W. Holden, “Identification of a virulence locus encoding a second type III secretion system in Salmonella typhimurium,” Proceedings of the National Academy of Sciences of the United States of America, vol. 93, no. 6, pp. 2593–2597, 1996.
- H. Ochman, F. C. Soncini, F. Solomon, and E. A. Groisman, “Identification of a pathogenicity island required for Salmonella survival in host cells,” Proceedings of the National Academy of Sciences of the United States of America, vol. 93, no. 15, pp. 7800–7804, 1996.
- A. Vazquez-Torres, Y. Xu, J. Jones-Carson et al., “Salmonella pathogenicity island 2-dependent evasion of the phagocyte NADPH oxidase,” Science, vol. 287, no. 5458, pp. 1655–1658, 2000.
- C. Tükel, M. Raffatellu, D. Chessa, R. P. Wilson, M. Akçelik, and A. J. Bäumler, “Neutrophil influx during non-typhoidal salmonellosis: Who is in the driver's seat?” FEMS Immunology and Medical Microbiology, vol. 46, no. 3, pp. 320–329, 2006.
- L. W. Lamps, “Pathology of food-borne infectious diseases of the gastrointestinal tract: an update,” Advances in anatomic pathology, vol. 10, no. 6, pp. 319–327, 2003.
- I. A. Onwuezobe, P. O. Oshun, and C. C. Odigwe, “Antimicrobials for treating symptomatic non-typhoidal Salmonella infection,” Cochrane Database of Systematic Reviews, vol. 11, Article ID CD001167, 2012.
- J. A. Ibarra and O. Steele-Mortimer, “Salmonella—the ultimate insider. Salmonella virulence factors that modulate intracellular survival,” Cellular Microbiology, vol. 11, no. 11, pp. 1579–1586, 2009.
- T. P. Moest and S. Méresse, “Salmonella T3SSs: Successful mission of the secret(ion) agents,” Current Opinion in Microbiology, vol. 16, no. 1, pp. 38–44, 2013.
- J. E. Galán and H. Wolf-Watz, “Protein delivery into eukaryotic cells by type III secretion machines,” Nature, vol. 444, no. 7119, pp. 567–573, 2006.
- R. Figueira and D. W. Holden, “Functions of the Salmonella pathogenicity island 2 (SPI-2) type III secretion system effectors,” Microbiology, vol. 158, no. 5, pp. 1147–1161, 2012.
- N. F. Brown, B. A. Vallance, B. K. Coombes, Y. Valdez, B. A. Coburn, and B. B. Finlay, “Salmonella pathogenicity island 2 is expressed prior to penetrating the intestine,” PLoS Pathogens, vol. 1, no. 3, pp. 252–258, 2005.
- M. N. Giacomodonato, S. Uzzau, D. Bacciu et al., “SipA, SopA, SopB, SopD, and SopE2 effector proteins of Salmonella enterica serovar Typhimurium are synthesized at late stages of infection in mice,” Microbiology, vol. 153, no. 4, pp. 1221–1228, 2007.
- T. Kubori, A. Sukhan, S.-I. Aizawa, and J. E. Galán, “Molecular characterization and assembly of the needle complex of the Salmonella typhimurium type III protein secretion system,” Proceedings of the National Academy of Sciences of the United States of America, vol. 97, no. 18, pp. 10225–10230, 2000.
- A. Kawamoto, Y. V. Morimoto, T. Miyata et al., “Common and distinct structural features of Salmonella injectisome and flagellar basal body,” Scientific Reports, vol. 3, article 3369, 2013.
- F. Que, S. Wu, and R. Huang, “Salmonella pathogenicity Island 1(SPI-1) at work,” Current Microbiology, vol. 66, no. 6, pp. 582–587, 2013.
- C. A. Lopez, S. E. Winter, F. Rivera-Chávez et al., “Phage-mediated acquisition of a type III secreted effector protein boosts growth of Salmonella by nitrate respiration,” mBio, vol. 3, no. 3, 2012.
- T. Edgren, Å. Forsberg, R. Rosqvist, and H. Wolf-Watz, “Type III secretion in Yersinia: injectisome or not?” PLoS Pathogens, vol. 8, no. 5, Article ID e1002669, 2012.
- R. D. Hayward and V. Koronakis, “Direct nucleation and bundling of actin by the SipC protein of invasive Salmonella,” EMBO Journal, vol. 18, no. 18, pp. 4926–4934, 1999.
- E. J. McGhie, R. D. Hayward, and V. Koronakis, “Control of actin turnover by a Salmonella invasion protein,” Molecular Cell, vol. 13, no. 4, pp. 497–510, 2004.
- C. V. Srikanth, R. Mercado-Lubo, K. Hallstrom, and B. A. McCormick, “Salmonella effector proteins and host-cell responses,” Cellular and Molecular Life Sciences, vol. 68, no. 22, pp. 3687–3697, 2011.
- L. C. Brawn, R. D. Hayward, and V. Koronakis, “Salmonella SPI1 effector SipA persists after entry and cooperates with a SPI2 effector to regulate phagosome maturation and intracellular replication,” Cell Host and Microbe, vol. 1, no. 1, pp. 63–75, 2007.
- M. Rosselin, I. Virlogeux-Payant, C. Roy et al., “Rck of Salmonella enterica, subspecies enterica serovar Enteritidis, mediates Zipper-like internalization,” Cell Research, vol. 20, no. 6, pp. 647–664, 2010.
- P. Velge, A. Wiedemann, M. Rosselin et al., “Multiplicity of Salmonella entry mechanisms, a new paradigm for Salmonella pathogenesis,” Microbiologyopen, vol. 1, no. 3, pp. 243–258, 2012.
- J. C. Patel and J. E. Galán, “Investigating the function of Rho family GTPases during Salmonella/host cell interactions,” Methods in Enzymology, vol. 439, pp. 145–158, 2008.
- C. A. Lee, M. Silva, A. M. Siber, A. J. Kelly, E. Galyov, and B. A. McCormick, “A secreted Salmonella protein induces a proinflammatory response in epithelial cells, which promotes neutrophil migration,” Proceedings of the National Academy of Sciences of the United States of America, vol. 97, no. 22, pp. 12283–12288, 2000.
- D. Hersh, D. M. Monack, M. R. Smith, N. Ghori, S. Falkow, and A. Zychlinsky, “The Salmonella invasin SipB induces macrophage apoptosis by binding to caspase-1,” Proceedings of the National Academy of Sciences of the United States of America, vol. 96, no. 5, pp. 2396–2401, 1999.
- F. A. Norris, M. P. Wilson, T. S. Wallis, E. E. Galyov, and P. W. Majerus, “SopB, a protein required for virulence of Salmonella dublin, is an inositol phosphate phosphatase,” Proceedings of the National Academy of Sciences of the United States of America, vol. 95, no. 24, pp. 14057–14059, 1998.
- L. S. Bertelsen, G. Paesold, S. L. Marcus, B. B. Finlay, L. Eckmann, and K. E. Barrett, “Modulation of chloride secretory responses and barrier function of intestinal epithelial cells by the Salmonella effector protein SigD,” The American Journal of Physiology—Cell Physiology, vol. 287, no. 4, pp. C939–C948, 2004.
- M. Hensel, J. E. Shea, C. Gleeson, M. D. Jones, E. Dalton, and D. W. Holden, “Simultaneous identification of bacterial virulence genes by negative selection,” Science, vol. 269, no. 5222, pp. 400–403, 1995.
- P. Mazurkiewicz, C. M. Tang, C. Boone, and D. W. Holden, “Signature-tagged mutagenesis: barcoding mutants for genome-wide screens,” Nature Reviews Genetics, vol. 7, no. 12, pp. 929–939, 2006.
- X. J. Yu, K. McGourty, M. Liu, K. E. Unsworth, and D. W. Holden, “pH sensing by intracellular Salmonella induces effector translocation,” Science, vol. 328, no. 5981, pp. 1040–1043, 2010.
- F. S. Mesquita, M. Thomas, M. Sachse, A. J. M. Santos, R. Figueira, and D. W. Holden, “The Salmonella deubiquitinase Ssel inhibits selective autophagy of cytosolic aggregates,” PLoS Pathogens, vol. 8, no. 6, Article ID e1002743, 2012.
- F. Bäckhed, R. E. Ley, J. L. Sonnenburg, D. A. Peterson, and J. I. Gordon, “Host-bacterial mutualism in the human intestine,” Science, vol. 307, no. 5717, pp. 1915–1920, 2005.
- J. I. Gordon, “Honor thy gut symbionts redux,” Science, vol. 336, no. 6086, pp. 1251–1253, 2012.
- W. B. Whitman, D. C. Coleman, and W. J. Wiebe, “Prokaryotes: The unseen majority,” Proceedings of the National Academy of Sciences of the United States of America, vol. 95, no. 12, pp. 6578–6583, 1998.
- D. C. Savage, “Microbial ecology of the gastrointestinal tract,” Annual Review of Microbiology, vol. 31, pp. 107–133, 1977.
- E. K. Costello, C. L. Lauber, M. Hamady, N. Fierer, J. I. Gordon, and R. Knight, “Bacterial community variation in human body habitats across space and time,” Science, vol. 326, no. 5960, pp. 1694–1697, 2009.
- P. J. Turnbaugh, R. E. Ley, M. A. Mahowald, V. Magrini, E. R. Mardis, and J. I. Gordon, “An obesity-associated gut microbiome with increased capacity for energy harvest,” Nature, vol. 444, no. 7122, pp. 1027–1031, 2006.
- J. O. Gebbers and J. A. Laissue, “Immunologic structures and functions of the gut,” Schweizer Archiv fur Tierheilkunde, vol. 131, no. 5, pp. 221–238, 1989.
- P. J. Turnbaugh and J. I. Gordon, “The core gut microbiome, energy balance and obesity,” Journal of Physiology, vol. 587, no. 17, pp. 4153–4158, 2009.
- J. Qin, R. Li, J. Raes et al., “A human gut microbial gene catalogue established by metagenomic sequencing,” Nature, vol. 464, no. 7285, pp. 59–65, 2010.
- P. B. Eckburg, E. M. Bik, C. N. Bernstein et al., “Microbiology: diversity of the human intestinal microbial flora,” Science, vol. 308, no. 5728, pp. 1635–1638, 2005.
- D. van der Waaij and J. M. Berghuis-de Vries, “Colonization resistance of the digestive tract in conventional and antibiotic-treated mice,” Journal of Hygiene, vol. 69, no. 3, pp. 405–411, 1971.
- G. D. Wu, J. Chen, C. Hoffmann et al., “Linking long-term dietary patterns with gut microbial enterotypes,” Science, vol. 334, no. 6052, pp. 105–108, 2011.
- L. A. David, C. F. Maurice, R. N. Carmody et al., “Diet rapidly and reproducibly alters the human gut microbiome,” Nature, vol. 505, no. 7484, pp. 559–563, 2014.
- J. J. Faith, J. L. Guruge, M. Charbonneau et al., “The long-term stability of the human gut microbiota,” Science, vol. 341, no. 6141, Article ID 1237439, 2013.
- L. Dethlefsen, S. Huse, M. L. Sogin, and D. A. Relman, “The pervasive effects of an antibiotic on the human gut microbiota, as revealed by deep 16S rRNA sequencing,” PLoS biology, vol. 6, no. 11, article e280, 2008.
- K. M. Ng, J. A. Ferreyra, S. K. Higginbottom et al., “Microbiota-liberated host sugars facilitate post-antibiotic expansion of enteric pathogens,” Nature, vol. 502, no. 7469, pp. 96–99, 2013.
- J. M. Blackwell, “Genetics and genomics in infectious disease susceptibility,” Trends in Molecular Medicine, vol. 7, no. 11, pp. 521–526, 2001.
- P. Kaiser, M. Diard, B. Stecher, and W.-D. Hardt, “The streptomycin mouse model for Salmonella diarrhea: functional analysis of the microbiota, the pathogen's virulence factors, and the host's mucosal immune response,” Immunological Reviews, vol. 245, no. 1, pp. 56–83, 2012.
- B. Stecher, A. J. Macpherson, S. Hapfelmeier, M. Kremer, T. Stallmach, and W. D. Hardt, “Comparison of Salmonella enterica serovar typhimurium colitis in germfree mice and mice pretreated with streptomycin,” Infection and Immunity, vol. 73, no. 6, pp. 3228–3241, 2005.
- S. Zhang, R. A. Kingsley, R. L. Santos et al., “Molecular pathogenesis of Salmonella enterica serotype typhimurium-induced diarrhea,” Infection and Immunity, vol. 71, no. 1, pp. 1–12, 2003.
- S. Hapfelmeier and W. D. Hardt, “A mouse model for S. typhimurium-induced enterocolitis,” Trends in Microbiology, vol. 13, no. 10, pp. 497–503, 2005.
- E. C. Martens, R. Roth, J. E. Heuser, and J. I. Gordon, “Coordinate regulation of glycan degradation and polysaccharide capsule biosynthesis by a prominent human gut symbiont,” Journal of Biological Chemistry, vol. 284, no. 27, pp. 18445–18457, 2009.
- P. Dharmani, V. Srivastava, V. Kissoon-Singh, and K. Chadee, “Role of intestinal mucins in innate host defense mechanisms against pathogens,” Journal of Innate Immunity, vol. 1, no. 2, pp. 123–135, 2009.
- Y. Ito, H. Moriwaki, Y. Muto, N. Kato, K. Watanabe, and K. Ueno, “Effect of lactulose on short-chain fatty acids and lactate production and on the growth of faecal flora, with special reference to Clostridium difficile,” Journal of Medical Microbiology, vol. 46, no. 1, pp. 80–84, 1997.
- L. E. J. Searle, A. Best, A. Nunez et al., “A mixture containing galactooligosaccharide, produced by the enzymic activity of bifidobacterium bifidum, reduces Salmonella enterica serovar typhimurium infection in mice,” Journal of Medical Microbiology, vol. 58, no. 1, pp. 37–48, 2009.
- K. Truusalu, R.-H. Mikelsaar, P. Naaber et al., “Eradication of Salmonella Typhimurium infection in a murine model of typhoid fever with the combination of probiotic Lactobacillus fermentum ME-3 and ofloxacin,” BMC Microbiology, vol. 8, article 132, 2008.
- L. Drago, M. R. Gismondo, A. Lombardi, C. De Haën, and L. Gozzini, “Inhibition of in vitro growth of enteropathogens by new Lactobacillus isolates of human intestinal origin,” FEMS Microbiology Letters, vol. 153, no. 2, pp. 455–463, 1997.
- A. M. Silva, F. H. F. Barbosa, R. Duarte, L. Q. Vieira, R. M. E. Arantes, and J. R. Nicoli, “Effect of Bifidobacterium longum ingestion on experimental salmonellosis in mice,” Journal of Applied Microbiology, vol. 97, no. 1, pp. 29–37, 2004.
- I. Gantois, R. Ducatelle, F. Pasmans et al., “Butyrate specifically down-regulates Salmonella pathogenicity island 1 gene expression,” Applied and Environmental Microbiology, vol. 72, no. 1, pp. 946–949, 2006.
- A. W. Walker, J. Ince, S. H. Duncan et al., “Dominant and diet-responsive groups of bacteria within the human colonic microbiota,” ISME Journal, vol. 5, no. 2, pp. 220–230, 2011.
- N. Kamada, G. Y. Chen, N. Inohara, and G. Núñez, “Control of pathogens and pathobionts by the gut microbiota,” Nature Immunology, vol. 14, no. 7, pp. 685–690, 2013.
- Y. Huang, M. Suyemoto, C. D. Garner, K. M. Cicconi, and C. Altier, “Formate acts as a diffusible signal to induce Salmonella invasion,” Journal of Bacteriology, vol. 190, no. 12, pp. 4233–4241, 2008.
- C. D. Garner, D. A. Antonopoulos, B. Wagner et al., “Perturbation of the small intestine microbial ecology by streptomycin alters pathology in a Salmonella enterica serovar typhimurium murine model of infection,” Infection and Immunity, vol. 77, no. 7, pp. 2691–2702, 2009.
- R. C. Charles, T. Sultana, M. M. Alam et al., “Identification of Immunogenic Salmonella enterica Serotype Typhi Antigens Expressed in Chronic Biliary Carriers of S. Typhi in Kathmandu, Nepal,” PLoS Neglected Tropical Diseases, vol. 7, no. 8, Article ID e2335, 2013.
- P. T. Desai, S. Porwollik, F. Long et al., “Evolutionary genomics of Salmonella enterica subspecies,” mBio, vol. 4, no. 2, Article ID e00579-12, 2013.
- K. Endt, B. Stecher, S. Chaffron et al., “The microbiota mediates pathogen clearance from the gut lumen after non-typhoidal Salmonella diarrhea,” PLoS Pathogens, vol. 6, no. 9, Article ID e01097, 2010.
- L. Maier, R. Vyas, C. D. Cordova et al., “Microbiota-derived hydrogen fuels Salmonella typhimurium invasion of the gut ecosystem,” Cell Host & Microbe, vol. 14, no. 6, pp. 641–651, 2013.
- B. Stecher, L. Maier, and W.-D. Hardt, “'Blooming' in the gut: How dysbiosis might contribute to pathogen evolution,” Nature Reviews Microbiology, vol. 11, no. 4, pp. 277–284, 2013.
- P. Thiennimitr, S. E. Winter, and A. J. Bäumler, “Salmonella, the host and its microbiota,” Current Opinion in Microbiology, vol. 15, no. 1, pp. 108–114, 2012.
- S. Hapfelmeier, K. Ehrbar, B. Stecher, M. Barthel, M. Kremer, and W.-D. Hardt, “Role of the Salmonella Pathogenicity Island 1 Effector Proteins SipA, SopB, SopE, and SopE2 in Salmonella enterica Subspecies 1 Serovar Typhimurium Colitis in Streptomycin-Pretreated Mice,” Infection and Immunity, vol. 72, no. 2, pp. 795–809, 2004.
- B. Stecher, R. Robbiani, A. W. Walker et al., “Salmonella enterica serovar typhimurium exploits inflammation to compete with the intestinal microbiota,” PLoS Biology, vol. 5, no. 10, pp. 2177–2189, 2007.
- A. J. Müller, C. Hoffmann, M. Galle et al., “The S. Typhimurium effector SopE induces caspase-1 activation in stromal cells to initiate gut inflammation,” Cell Host & Microbe, vol. 6, no. 2, pp. 125–136, 2009.
- B. M. Fournier and C. A. Parkos, “The role of neutrophils during intestinal inflammation,” Mucosal Immunology, vol. 5, no. 4, pp. 354–366, 2012.
- S. E. Winter, P. Thiennimitr, M. G. Winter et al., “Gut inflammation provides a respiratory electron acceptor for Salmonella,” Nature, vol. 467, no. 7314, pp. 426–429, 2010.
- W. D. Hardt, L. M. Chen, K. E. Schuebel, X. R. Bustelo, and J. E. Galán, “S. typhimurium Encodes an activator of Rho GTPases that induces membrane ruffling and nuclear responses in host cells,” Cell, vol. 93, no. 5, pp. 815–826, 1998.
- S. E. Winter, M. G. Winter, M. N. Xavier et al., “Host-derived nitrate boosts growth of E. coli in the inflamed gut,” Science, vol. 339, no. 6120, pp. 708–711, 2013.
- Y. Bertin, J. P. Girardeau, F. Chaucheyras-Durand et al., “Enterohaemorrhagic Escherichia coli gains a competitive advantage by using ethanolamine as a nitrogen source in the bovine intestinal content,” Environmental Microbiology, vol. 13, no. 2, pp. 365–377, 2011.
- P. Thiennimitr, S. E. Winter, M. G. Winter et al., “Intestinal inflammation allows Salmonella to use ethanolamine to compete with the microbiota,” Proceedings of the National Academy of Sciences of the United States of America, vol. 108, no. 42, pp. 17480–17485, 2011.
- F. Rivera-Chávez, S. E. Winter, C. A. Lopez et al., “Salmonella uses energy taxis to benefit from intestinal inflammation,” PLoS Pathogens, vol. 9, no. 4, Article ID e1003267, 2013.
- K. L. Meibom, M. Blokesch, N. A. Dolganov, C.-Y. Wu, and G. K. Schoolnik, “Microbiology: chitin induces natural competence in vibrio cholerae,” Science, vol. 310, no. 5755, pp. 1824–1827, 2005.
- C. A. Van Reenen and L. M. T. Dicks, “Horizontal gene transfer amongst probiotic lactic acid bacteria and other intestinal microbiota: what are the possibilities? A review,” Archives of Microbiology, vol. 193, no. 3, pp. 157–168, 2011.
- M. Begley, C. Hill, and C. G. M. Gahan, “Bile salt hydrolase activity in probiotics,” Applied and Environmental Microbiology, vol. 72, no. 3, pp. 1729–1738, 2006.
- B. V. Jones, F. Sun, and J. R. Marchesi, “Comparative metagenomic analysis of plasmid encoded functions in the human gut microbiome,” BMC Genomics, vol. 11, no. 1, article 46, 2010.
- T. Dagan, Y. Artzy-Randrup, and W. Martin, “Modular networks and cumulative impact of lateral transfer in prokaryote genome evolution,” Proceedings of the National Academy of Sciences of the United States of America, vol. 105, no. 29, pp. 10039–10044, 2008.
- M. Llosa, G. Schröder, and C. Dehio, “New perspectives into bacterial DNA transfer to human cells,” Trends in Microbiology, vol. 20, no. 8, pp. 355–359, 2012.
- M. S. Dorer, J. Fero, and N. R. Salama, “DNA damage triggers genetic exchange in Helicobacter pylori,” PLoS pathogens, vol. 6, no. 7, Article ID e1001026, 2010.
- S. Mirold, W. Rabsch, M. Rohde et al., “Isolation of a temperate bacteriophage encoding the type III effector protein SopE from an epidemic Salmonella typhimurium strain,” Proceedings of the National Academy of Sciences of the United States of America, vol. 96, no. 17, pp. 9845–9850, 1999.
- B. A. Duerkop, C. V. Clements, D. Rollins, J. L. M. Rodrigues, and L. V. Hooper, “A composite bacteriophage alters colonization by an intestinal commensal bacterium,” Proceedings of the National Academy of Sciences of the United States of America, vol. 109, no. 43, pp. 17621–17626, 2012.
- G. Peterson, A. Kumar, E. Gart, and S. Narayanan, “Catecholamines increase conjugative gene transfer between enteric bacteria,” Microbial Pathogenesis, vol. 51, no. 1-2, pp. 1–8, 2011.
- B. Stecher, R. Denzler, L. Maier et al., “Gut inflammation can boost horizontal gene transfer between pathogenic and commensal Enterobacteriaceae,” Proceedings of the National Academy of Sciences of the United States of America, vol. 109, no. 4, pp. 1269–1274, 2012.
- A. M. Spees, T. Wangdi, C. A. Lopez et al., “Streptomycin-induced inflammation enhances Escherichia coli gut colonization through nitrate respiration,” mBio, vol. 4, no. 4, 2013.
- P. Garai, D. P. Gnanadhas, and D. Chakravortty, “Salmonella enterica serovars typhimurium and typhi as model organisms: revealing paradigm of host-pathogen interactions,” Virulence, vol. 3, no. 4, pp. 377–388, 2012.
- A. Lahiri, P. Das, and D. Chakravortty, “Engagement of TLR signaling as adjuvant: Towards smarter vaccine and beyond,” Vaccine, vol. 26, no. 52, pp. 6777–6783, 2008.
- S. M. Bueno, S. Riquelme, C. A. Riedel, and A. M. Kalergis, “Mechanisms used by virulent Salmonella to impair dendritic cell function and evade adaptive immunity,” Immunology, vol. 137, no. 1, pp. 28–36, 2012.
- N. Arpaia, J. Godec, L. Lau et al., “TLR signaling is required for Salmonella typhimurium virulence,” Cell, vol. 144, no. 5, pp. 675–688, 2011.
- P. Broz, M. B. Ohlson, and D. M. Monack, “Innate immune response to Salmonella typhimurium, a model enteric pathogen,” Gut Microbes, vol. 3, no. 2, pp. 62–70, 2012.
- P. Das, A. Lahiri, A. Lahiri, and D. Chakravortty, “Modulation of the arginase pathway in the context of microbial pathogenesis: a metabolic enzyme moonlighting as an immune modulator,” PLoS Pathogens, vol. 6, no. 6, Article ID e1000899, 2010.
- J. Y. Chau, C. M. Tiffany, S. Nimishakavi et al., “Malaria-associated L-Arginine deficiency induces mast cell-associated disruption to intestinal barrier defenses against non-typhoidal Salmonella bacteremia,” Infection and Immunity, vol. 81, no. 10, pp. 3515–3526, 2013.
- J. H. Fritz, “Arginine cools the inflamed gut,” Infection and Immunity, vol. 81, no. 10, pp. 3500–3502, 2013.
- D. Osman and J. S. Cavet, “Metal sensing in Salmonella: implications for pathogenesis,” Advances in Microbial Physiology, vol. 58, pp. 176–232, 2011.
- M. A. Fischbach, H. Lin, D. R. Liu, and C. T. Walsh, “How pathogenic bacteria evade mammalian sabotage in the battle for iron,” Nature Chemical Biology, vol. 2, no. 3, pp. 132–138, 2006.
- M. Raffatellu, M. D. George, Y. Akiyama et al., “Lipocalin-2 resistance confers an advantage to Salmonella enterica serotype Typhimurium for growth and survival in the inflamed intestine,” Cell Host and Microbe, vol. 5, no. 5, pp. 476–486, 2009.
- S. Chakraborty, S. Kaur, S. Guha, and S. K. Batra, “The multifaceted roles of neutrophil gelatinase associated lipocalin (NGAL) in inflammation and cancer,” Biochimica et Biophysica Acta, vol. 1826, no. 1, pp. 129–169, 2012.
- A. J. Bäumler, R. M. Tsolis, A. W. M. van der Velden, I. Stojiljkovic, S. Anic, and F. Heffron, “Identification of a new iron regulated locus of Salmonella typhi,” Gene, vol. 183, no. 1-2, pp. 207–213, 1996.
- A. J. Bäumler, T. L. Norris, T. Lasco et al., “IroN, a novel outer membrane siderophore receptor characteristic of Salmonella enterica,” Journal of Bacteriology, vol. 180, no. 6, pp. 1446–1453, 1998.
- B. Bister, D. Bischoff, G. J. Nicholson et al., “The structure of salmochelins: C-glucosylated enterobactins of Salmonella enterica,” BioMetals, vol. 17, no. 4, pp. 471–481, 2004.
- K. Hantke, G. Nicholson, W. Rabsch, and G. Winkelmann, “Salmochelins, siderophores of Salmonella enterica and uropathogenic Escherichia coli strains, are recognized by the outer membrane receptor IroN,” Proceedings of the National Academy of Sciences of the United States of America, vol. 100, no. 7, pp. 3677–3682, 2003.
- W. Rabsch, W. Voigt, R. Reissbrodt, R. M. Tsolis, and A. J. Bäumler, “Salmonella typhimurium IroN and FepA proteins mediate uptake of enterobactin but differ in their specificity for other siderophores,” Journal of Bacteriology, vol. 181, no. 11, pp. 3610–3612, 1999.
- M. Zhu, M. Valdebenito, G. Winkelmann, and K. Hantke, “Functions of the siderophore esterases IroD and IroE in iron-salmochelin utilization,” Microbiology, vol. 151, no. 7, pp. 2363–2372, 2005.
- J. Z. Liu, S. Jellbauer, A. J. Poe et al., “Zinc sequestration by the neutrophil protein calprotectin enhances Salmonella growth in the inflamed gut,” Cell Host & Microbe, vol. 11, no. 3, pp. 227–239, 2012.
- A. NISSLE, “On coli antagonism, dysbacteria and coli therapy,” Medizinische Monatsschrift, vol. 13, pp. 489–491, 1959.
- J. Henker, M. Laass, B. M. Blokhin et al., “The probiotic Escherichia coli strain Nissle 1917 (EcN) stops acute diarrhoea in infants and toddlers,” European Journal of Pediatrics, vol. 166, no. 4, pp. 311–318, 2007.
- E. Deriu, J. Z. Liu, M. Pezeshki et al., “Probiotic bacteria reduce Salmonella typhimurium intestinal colonization by competing for iron,” Cell Host and Microbe, vol. 14, no. 1, pp. 26–37, 2013.
- S. Schauder and B. L. Bassler, “The languages of bacteria,” Genes and Development, vol. 15, no. 12, pp. 1468–1480, 2001.
- P. Williams, “Quorum sensing, communication and cross-kingdom signalling in the bacterial world,” Microbiology, vol. 153, no. 12, pp. 3923–3938, 2007.
- L. C. M. Antunes, R. B. R. Ferreira, M. M. C. Buckner, and B. B. Finlay, “Quorum sensing in bacterial virulence,” Microbiology, vol. 156, no. 8, pp. 2271–2282, 2010.
- W. L. Ng and B. L. Bassler, “Bacterial quorum-sensing network architectures,” Annual Review of Genetics, vol. 43, pp. 197–222, 2009.
- M. M. Kendall and V. Sperandio, “Quorum sensing by enteric pathogens,” Current Opinion in Gastroenterology, vol. 23, no. 1, pp. 10–15, 2007.
- M. H. Karavolos, K. Winzer, P. Williams, and C. M. A. Khan, “Pathogen espionage: multiple bacterial adrenergic sensors eavesdrop on host communication systems,” Molecular Microbiology, vol. 87, no. 3, pp. 455–465, 2013.
- J. L. Dyszel, J. N. Smith, D. E. Lucas et al., “Salmonella enterica serovar typhimurium can detect acyl homoserine lactone production by Yersinia enterocolitica in mice,” Journal of Bacteriology, vol. 192, no. 1, pp. 29–37, 2010.
- J. N. Smith, J. L. Dyszel, J. A. Soares et al., “SdiA, an N-acylhomoserine lactone receptor, becomes active during the transit of Salmonella enterica through the gastrointestinal tract of turtles,” PLoS ONE, vol. 3, no. 7, Article ID e2826, 2008.
- V. Sperandio, “SdiA sensing of acyl-homoserine lactones by enterohemorrhagic E. coli (EHEC) serotype O157:H7 in the bovine rumen,” Gut microbes, vol. 1, no. 6, pp. 432–435, 2010.
- M. C. Swearingen, A. Sabag-Daigle, and B. M. M. Ahmer, “Are there acyl-homoserine lactones within mammalian intestines?” Journal of Bacteriology, vol. 195, no. 2, pp. 173–179, 2013.
- S. T. Miller, K. B. Xavier, S. R. Campagna et al., “Salmonella typhimurium recognizes a chemically distinct form of the bacterial quorum-sensing signal AI-2,” Molecular Cell, vol. 15, no. 5, pp. 677–687, 2004.
- M. G. Surette, M. B. Miller, and B. L. Bassler, “Quorum sensing in Escherichia coli, Salmonella typhimurium, and Vibrio harveyi: a new family of genes responsible for autoinducer production,” Proceedings of the National Academy of Sciences of the United States of America, vol. 96, no. 4, pp. 1639–1644, 1999.
- K. Winzer, K. R. Hardie, N. Burgess et al., “LuxS: its role in central metabolism and the in vitro synthesis of 4-hydroxy-5-methyl-3(2H)-furanone,” Microbiology, vol. 148, no. 4, pp. 909–922, 2002.
- M. E. Taga, S. T. Miller, and B. L. Bassler, “Lsr-mediated transport and processing of Al-2 in Salmonella typhimurium,” Molecular Microbiology, vol. 50, no. 4, pp. 1411–1427, 2003.
- K. B. Xavier and B. L. Bassler, “Regulation of uptake and processing of the quorum-sensing autoinducer AI-2 in Escherichia coli,” Journal of Bacteriology, vol. 187, no. 1, pp. 238–248, 2005.
- S. C. J. de Keersmaeckert, C. Varszegi, N. Van Boxel et al., “Chemical synthesis of (S)-4,5-dihydroxy-2,3-pentanedione, a bacterial signal molecule precursor, and validation of its activity in Salmonella typhimurium,” Journal of Biological Chemistry, vol. 280, no. 20, pp. 19563–19568, 2005.
- M. H. Karavolos, D. M. Bulmer, K. Winzer et al., “LuxS affects flagellar phase variation independently of quorum sensing in Salmonella enterica serovar typhimurium,” Journal of Bacteriology, vol. 190, no. 2, pp. 769–771, 2008.
- G. Kint, K. A. J. Sonck, G. Schoofs, D. De Coster, J. Vanderleyden, and S. C. J. de Keersmaecker, “2D proteome analysis initiates new Insights on the Salmonella Typhimurium LuxS protein,” BMC Microbiology, vol. 9, article 198, 2009.
- G. Kint, D. de Coster, K. Marchal, J. Vanderleyden, and S. C. de Keersmaecker, “The small regulatory RNA molecule MicA is involved in Salmonella enterica serovar Typhimurium biofilm formation,” BMC Microbiology, vol. 10, article 276, 2010.
- S. Redanz, K. Standar, A. Podbielski, and B. Kreikemeyer, “Heterologous expression of sahH reveals that biofilm formation is autoinducer-2-independent in Streptococcus sanguinis but is associated with an intact activated methionine cycle,” Journal of Biological Chemistry, vol. 287, no. 43, pp. 36111–36122, 2012.
- P. R. Jesudhasan, M. L. Cepeda, K. Widmer et al., “Transcriptome analysis of genes controlled by luxS/Autoinducer-2 in Salmonella enterica serovar typhimurium,” Foodborne Pathogens and Disease, vol. 7, no. 4, pp. 399–410, 2010.
- V. Sperandio, A. G. Torres, B. Jarvis, J. P. Nataro, and J. B. Kaper, “Bacteria-host communication: the language of hormones,” Proceedings of the National Academy of Sciences of the United States of America, vol. 100, no. 15, pp. 8951–8956, 2003.
- M. Walters, M. P. Sircili, and V. Sperandio, “AI-3 synthesis is not dependent on luxS in Escherichia coli,” Journal of Bacteriology, vol. 188, no. 16, pp. 5668–5681, 2006.
- L. C. Martha Antunes, L. Q. Ferreira, E. O. Ferreira et al., “Bacteroides species produce Vibrio harveyi autoinducer 2-related molecules,” Anaerobe, vol. 11, no. 5, pp. 295–301, 2005.
- R. J. Peixoto, K. R. Miranda, E. O. Ferreira et al., “Production of AI-2 is mediated by the S-ribosylhomocystein lyase gene luxS in Bacteroides fragilis and Bacteroides vulgatus,” Journal of Basic Microbiology, 2013.
- J. L. Botsford and R. D. Demoss, “Escherichia coli tryptophanase in the enteric environment,” Journal of Bacteriology, vol. 109, no. 1, pp. 74–80, 1972.
- E. Zuccato, M. Venturi, G. Di Leo et al., “Role of bile acids and metabolic activity of colonic bacteria in increased risk of colon cancer after cholecystectomy,” Digestive Diseases and Sciences, vol. 38, no. 3, pp. 514–519, 1993.
- E. Nikaido, E. Giraud, S. Baucheron et al., “Effects of indole on drug resistance and virulence of Salmonella enterica serovar Typhimurium revealed by genome-wide analyses,” Gut Pathogens, vol. 4, no. 1, article 5, 2012.
- N. M. Vega, K. R. Allison, A. S. Khalil, and J. J. Collins, “Signaling-mediated bacterial persister formation,” Nature Chemical Biology, vol. 8, no. 5, pp. 431–433, 2012.
- T. Bansal, R. C. Alaniz, T. K. Wood, and A. Jayaraman, “The bacterial signal indole increases epithelial-cell tight-junction resistance and attenuates indicators of inflammation,” Proceedings of the National Academy of Sciences of the United States of America, vol. 107, no. 1, pp. 228–233, 2010.
- M. Lyte, B. P. Arulanandam, and C. D. Frank, “Production of Shiga-like toxins by Escherichia coli O157:H7 can be influenced by the neuroendocrine hormone norepinephrine,” Journal of Laboratory and Clinical Medicine, vol. 128, no. 4, pp. 392–398, 1996.
- M. Lyte, “Microbial endocrinology and infectious disease in the 21st century,” Trends in Microbiology, vol. 12, no. 1, pp. 14–20, 2004.
- P. P. E. Freestone, S. M. Sandrini, R. D. Haigh, and M. Lyte, “Microbial endocrinology: how stress influences susceptibility to infection,” Trends in Microbiology, vol. 16, no. 2, pp. 55–64, 2008.
- Y. Asano, T. Hiramoto, R. Nishino et al., “Critical role of gut microbiota in the production of biologically active, free catecholamines in the gut lumen of mice,” The American Journal of Physiology—Gastrointestinal and Liver Physiology, vol. 303, no. 11, pp. G1288–G1295, 2012.
- D. A. Rasko, C. G. Moreira, R. L. de et al., “Targeting QseC signaling and virulence for antibiotic development,” Science, vol. 321, no. 5892, pp. 1078–1080, 2008.
- A. R. Pacheco and V. Sperandio, “Inter-kingdom signaling: chemical language between bacteria and host,” Current Opinion in Microbiology, vol. 12, no. 2, pp. 192–198, 2009.
- M. H. Karavolos, D. M. Bulmer, H. Spencer et al., “Salmonella Typhi sense host neuroendocrine stress hormones and release the toxin haemolysin E,” EMBO Reports, vol. 12, no. 3, pp. 252–258, 2011.
- H. Spencer, M. H. Karavolos, D. M. Bulmer et al., “Genome-wide transposon mutagenesis identifies a role for host neuroendocrine stress hormones in regulating the expression of virulence genes in Salmonella,” Journal of Bacteriology, vol. 192, no. 3, pp. 714–724, 2010.
- M. H. Karavolos, H. Spencer, D. M. Bulmer et al., “Adrenaline modulates the global transcriptional profile of Salmonella revealing a role in the antimicrobial peptide and oxidative stress resistance responses,” BMC Genomics, vol. 9, article 458, 2008.
- K. Kawasaki, R. K. Ernst, and S. I. Miller, “3-O-deacylation of lipid A by PagL, a PhoP/PhoQ-regulated deacylase of Salmonella typhimurium, modulates signaling through Toll-like receptor 4,” Journal of Biological Chemistry, vol. 279, no. 19, pp. 20044–20048, 2004.
- M. H. Karavolos, P. Williams, and C. M. A. Khan, “Interkingdom crosstalk: host neuroendocrine stress hormones drive the hemolytic behavior of Salmonella typhi,” Virulence, vol. 2, no. 4, pp. 371–374, 2011.
- J. Xu, M. K. Bjursell, J. Himrod et al., “A genomic view of the human-Bacteroides thetaiotaomicron symbiosis,” Science, vol. 299, no. 5615, pp. 2074–2076, 2003.
- C. Robbe, C. Capon, B. Coddeville, and J. C. Michalski, “Structural diversity and specific distribution of O-glycans in normal human mucins along the intestinal tract,” Biochemical Journal, vol. 384, no. 2, pp. 307–316, 2004.
- A. R. Pacheco, M. M. Curtis, J. M. Ritchie et al., “Fucose sensing regulates bacterial intestinal colonization,” Nature, vol. 491, no. 7427, pp. 113–117, 2012.
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