Browse Subject Areas

Click through the PLOS taxonomy to find articles in your field.

For more information about PLOS Subject Areas, click here.

  • Loading metrics

Cell Walls of Saccharomyces cerevisiae Differentially Modulated Innate Immunity and Glucose Metabolism during Late Systemic Inflammation

Cell Walls of Saccharomyces cerevisiae Differentially Modulated Innate Immunity and Glucose Metabolism during Late Systemic Inflammation

  • Bushansingh Baurhoo, 
  • Peter Ferket, 
  • Chris M. Ashwell, 
  • Jean de Oliviera, 
  • Xin Zhao



Salmonella causes acute systemic inflammation by using its virulence factors to invade the intestinal epithelium. But, prolonged inflammation may provoke severe body catabolism and immunological diseases. Salmonella has become more life-threatening due to emergence of multiple-antibiotic resistant strains. Mannose-rich oligosaccharides (MOS) from cells walls of Saccharomyces cerevisiae have shown to bind mannose-specific lectin of Gram-negative bacteria including Salmonella, and prevent their adherence to intestinal epithelial cells. However, whether MOS may potentially mitigate systemic inflammation is not investigated yet. Moreover, molecular events underlying innate immune responses and metabolic activities during late inflammation, in presence or absence of MOS, are unknown.

Methods and Principal Findings

Using a Salmonella LPS-induced systemic inflammation chicken model and microarray analysis, we investigated the effects of MOS and virginiamycin (VIRG, a sub-therapeutic antibiotic) on innate immunity and glucose metabolism during late inflammation. Here, we demonstrate that MOS and VIRG modulated innate immunity and metabolic genes differently. Innate immune responses were principally mediated by intestinal IL-3, but not TNF-α, IL-1 or IL-6, whereas glucose mobilization occurred through intestinal gluconeogenesis only. MOS inherently induced IL-3 expression in control hosts. Consequent to LPS challenge, IL-3 induction in VIRG hosts but not differentially expressed in MOS hosts revealed that MOS counteracted LPS's detrimental inflammatory effects. Metabolic pathways are built to elucidate the mechanisms by which VIRG host's higher energy requirements were met: including gene up-regulations for intestinal gluconeogenesis (PEPCK) and liver glycolysis (ENO2), and intriguingly liver fatty acid synthesis through ATP citrate synthase (CS) down-regulation and ATP citrate lyase (ACLY) and malic enzyme (ME) up-regulations. However, MOS host's lower energy demands were sufficiently met through TCA citrate-derived energy, as indicated by CS up-regulation.


MOS terminated inflammation earlier than VIRG and reduced glucose mobilization, thus representing a novel biological strategy to alleviate Salmonella-induced systemic inflammation in human and animal hosts.


Salmonella is a leading human food-borne pathogen, worldwide [1]. The pathogen invades the intestinal epithelium by using its specialized Type III secretory systems (T3SS) to cause acute systemic or extra-intestinal inflammation [2]. Indeed, the intestine is the portal of entry through which Salmonella triggers systemic infections. However, although life-threatening, treatment of Salmonella-induced systemic inflammation has received very little interests in scientific investigations. The disease is frequently caused by consumption of undercooked contaminated poultry meat and meat products [3], which accidentally occur upon exposure to intestine-residing Salmonella during chicken processing.

Over decades, low doses of sub-therapeutic antibiotics such as virginiamycin (VIRG) have been administered daily in diets of food-producing animals, including poultry, to control intestinal pathogens. Unlike therapeutic antibiotics, sub-therapeutic antibiotics are macromolecules that exert localized bactericidal effects in the intestines only. However, according to the World Health Organization (WHO), such practice has debatably been associated with emergence of multiple antibiotic-resistant strains of Salmonella [4]. Today, not only has Salmonella become more difficult to control in poultry production, but antibiotic treatment of Salmonella-induced gastrointestinal and systemic infections has become less successful among hospitalized patients, causing higher death rates [1], [4]. Therefore, the development of natural immuno-modulators that can prevent or treat Salmonella infections in both poultry and humans is highly desirable. Evidence exist that mannose-rich oligosaccharides (MOS), purified from cells walls of Saccharomyces cerevisiae, competitively binds mannose-specific lectin, namely FimH, of Gram-negative bacteria expressing the Type 1 fimbriae, including Salmonella, thereby reducing their adherence to mannose-containing glycoprotein receptors on intestinal epithelial cells in humans and chickens [5], [6].

Innate immunity represents the first line of immune defense against invading pathogens in both mammals and avian species. Extracellular Toll-like receptor 4 (TLR-4) of innate immune cells, including macrophages and dendritic cells, recognizes the LPS-endotoxin in outer membranes of Gram-negative bacteria [7]. The engagement of LPS to TLR-4 triggers a cascade of transduction signaling resulting in inflammatory responses characterized by secretion of pro-inflammatory cytokines, including IL-1 and IL-6 that orchestrate pathogen clearance [8]. But, innate immune responses must be regulated exceptionally tightly because high IL-1 and IL-6 levels cause fever, anorexia and bodyweight (BW) losses [9], [10], catabolism of skeletal muscles [11][13] and adipose tissues [14], and immunological diseases [15] in chickens, rats and humans. Therefore, it is clear that an ideal immune response would be one that can clear pathogens or antigens and be terminated soon after infection. However, despite significant advances in our understanding about inflammatory responses, molecular events of innate immunity and metabolic activities during the period of late inflammation are still not clear. Moreover, whether modulation of intestinal mucosal immunity due to dietary MOS may suppress Salmonella-induced systemic inflammation and reduce nutrient mobilization is unknown. The regulatory immune responses between intestinal mucosal and systemic immunity is well recognized [16], [17]. Therefore, considering the human health havoc due to sub-therapeutic antibiotic utilization among food-producing animals, this study evaluated the effects of MOS and sub-therapeutic antibiotics on innate immunity and nutrient metabolism during late Salmonella LPS-induced systemic inflammation.

The experiment reported herein, conducted in a chicken model, a frequently utilized biological model in nutrigenomic scientific investigations [18], and using chicken-specific microarrays, reveals that MOS and the VIRG antibiotic differently regulated expressions of genes involved in innate immunity and metabolic pathways during late systemic inflammation. Innate immune responses were principally mediated by intestinal IL-3, but not IL-1 or IL-6. In contrast to VIRG, MOS inherently induced innate immune responses in non-challenged control hosts. Interestingly, however, MOS terminated innate immune responses earlier than VIRG and reduced glucose mobilization.


LPS induced pathological symptoms, reduced feed intake and BW, and increased liver size in MOS- and VIRG-fed chickens. However, to make a clear distinction between the effects of MOS and VIRG among hosts within the physiological (non-challenged controls) and inflammatory (LPS-challenged) conditions, we relied on microarray results that detailed the coordinately regulated biological mechanisms underlying innate immunity and nutrient metabolism. Tissue-specific RNA extracted from the intestines, liver and skeletal muscles at 24 h post-LPS challenge were analyzed using chicken-specific microarrays. All data files from this experiment have been deposited into the MIAME compliant Gene Expression Omnibus (GEO) database, (accession no. GSE28959).

LPS induced clinical symptoms in antibiotic- and MOS-fed chickens

To provoke a systemic inflammatory response, chickens were injected i.p. with a sublethal dose of LPS (3 ml of 100 mg LPS/L). The reaction to LPS is a well-characterized innate immune response [19]. Whether hosts were fed MOS or VIRG, LPS caused symptoms of drowsiness, lethargy, ruffled feathers, moderate diarrhea, starvation and withdrawal from water at 6 h post-LPS injection, thus demonstrating success of our challenge model. These clinical signs of innate immune response were most evident around 8 h after LPS injection. Clinical and behavioral changes due to LPS injection have previously been reported in different animal species, including chickens [9]. No signs of inflammatory responses were observed among non-challenged control hosts. To assess pathological changes further, body temperatures were measured at 0, 2, 4, 6, 8, 12, 24 and 48 h post-LPS injection. Body temperature was similar among all hosts prior (0 h) to LPS challenge (Figure S1A). But, LPS markedly increased body temperatures of MOS- and VIRG-fed hosts after 4 h of LPS challenge, and this effect persisted through 24 h (Figure S1A and B). After 48 h, however, all hosts regained their homeostatic state after termination of inflammatory responses (Figure S1A and B).

LPS reduced feed intake and bodyweight gain, and increased liver weight in antibiotic- and MOS-fed chickens

LPS markedly reduced feed intake at 12 h (Figure S2A), but not at 24 and 48 h, post-challenge despite VIRG and MOS supplementations. In addition, LPS's effects in reducing feed consumption and inducing profuse diarrhea at 12 h led to severe loss in BW gain (growth) (Figure S3A and C). However, depressed BW gain persisted through 24 and 48 h post-LPS challenge. On the other hand, increased liver weights were observed at 12 and 24 h among LPS-challenged hosts (Figure S4A and C). But, the more profound increase in liver weights that occurred after 12 h rather than 24 h (+0.66% vs +0.40% of BW) indicated that higher liver metabolic activities might have occurred at 12 h post-LPS challenge responsive to host's higher energy demands. Moreover, given the similarities in body temperatures, feed intake, and liver weights between LPS-challenge and non-challenge control hosts, it is clear that inflammatory responses were abated at 48 h post-LPS challenge. All of these findings indicated that inflammatory responses were more intense earlier than 24 h post-LPS challenge. Therefore, based on the similarity in feed intake, depressed growth and increased liver weights, but persistence in elevated body temperatures, we concluded that 24 h post-LPS treatment corresponded to late inflammation.

Main Effects: LPS increased innate immune responses

Our results revealed that LPS significantly increased innate immune responses in intestinal tissues (Table 1) characterized by IL-3 up-regulation, and down-regulation of the gene for zinc finger CCCH-type containing 15 (ZC3H15), which negatively regulates macrophage activation [20]. Additionally, the gene coding for the signal transducer and activator of transcription 2 (STAT2), a signaling pathway that augments macrophage's phagocytic activities against pathogenic bacteria by inducing inducible nitric oxide synthase (iNOS) and lysosomal enzymes [21], was induced in the liver. But, down-regulation of genes were observed for TLR 2 precursor (TLR2-2) that also recognizes and binds LPS [22], gallinacin-1 alpha (Gal-1), a wide spectrum antimicrobial peptide functionally equivalent to human β-defensins [23], and putative CXCR1, an IL-8 receptor that binds the IL-8 chemoattractant expressed by macrophages, monocytes and neutrophils. Indeed, gene expression for 2′–5′-oligoadenylate synthetase A (OAS*A), which is involved in viral RNA cleavage inhibiting IFN-γ-mediated viral infections [24], was intestinally down-regulated in the absence of viral infection. However, differential immune gene expressions as observed in the intestines and liver were not detected in muscle tissues.

Table 1. Genes identified as differentially expressed due to main LPS effects1.

Main Effects: LPS increased glucose mobilization and modified fatty acid metabolism

During acute inflammation, starvation alters host's carbohydrate, protein and fat metabolisms that are orchestrated by synergistically-operated pro-inflammatory cytokines, to meet the body's energy requirements. Subsequent to rapid glucose absorption and oxidative utilization, blood glucose level is maintained by liver glycogenolysis, catabolism of skeletal muscles that generates and mobilizes amino acids for liver gluconeogenesis [12], [13], and catabolism of adipose tissues that triggers liver lipolysis [14].

However, here, we observed that glucose mobilization occurred differently during late inflammation than during immunologically non-challenged conditions. LPS significantly increased intestinal gluconeogenesis by increasing gene expression for phosphoenolpyruvate carboxykinase 1 (PEPCK), a key gluconeogenic enzyme that synthesizes phosphoenolpyruvate from oxaloacetate (Table 1). Evidently, intestinal glycolysis and cholesterol synthesis were repressed as indicated by gene down-regulations for phosphopyruvate hydratase (ENO2), which converts 2-phosphoglycerate into phosphoenolpyruvate, and 3-hydroxy-3-methylglutaryl-CoA reductase (HMGCR), which catalyzes the rate-limiting step in the mevalonate pathway converting 3-hydroxy-3-methylglutaryl-CoA (HMG-CoA) into mevalonate [25], respectively. The high rates of glucose synthesis and glucose trafficking across intestinal epithelial cells enhanced intestinal contractions as indicated by myosin heavy polypeptide 7 cardiac muscle (MYH7) and myosin light polypeptide 9 regulatory (MYL9) up-regulations [26]. Contrary to expectations, gluconeogenesis did not occur in the liver. Intriguingly, LPS up-regulated genes coding for malic enzyme (ME), a key enzyme involved in fatty acid synthesis catalyzing the oxidative decarboxylation of malate to pyruvate, NADPH and carbon dioxide [27], and enoyl-CoA hydratase (EHHADH), a key enzyme involved in β-oxidation of fatty acids [28]. Therefore, metabolic energy to support late inflammation was derived mostly from increased fatty acid de-novo biosynthesis followed by its catabolism. Unexpectedly, LPS up-regulated gene for 5′-AMP-activated protein kinase gamma 2 (PRKAG2), a low energy sensor that represses acetyl-CoA carboxylase and HMG-CoA reductase to inhibit fatty acid and cholesterol biosynthesis, respectively [29]. In muscle tissues, down-regulation of the gene for 6-phosphofructokinase (PFKM), a regulatory enzyme that converts fructose-6-phosphate into fructose-1,6-biphosphate, suppressed the glycolytic pathway, whereas atrial natriuretic factor precursor (NPPA) up-regulation caused vasodilatation to increase blood flow [30]. Taken together, all these findings reveal a clear disassociation between glucose mobilization and the biosynthesis and β-oxidation of fatty acids. These discrepancies could be attributed to MOS's immune-stimulatory effects among non-challenged control hosts, as discussed later.

MOS increased innate immune responses in non-challenged control chickens

Because MOS increases Salmonella and E. coli clearance of the intestines [5], we thought that MOS may suppress innate immune responses under inflammatory conditions rather than VIRG thereby reducing catabolism of body reserves. However, MOS significantly increased innate immune responses among non-challenged control hosts than VIRG. For instance, several innate immune genes were induced by MOS in the intestines, including IL-3, TLR-3, TLR2-2 and Gal-1 (Table 2). Moreover MOS up-regulated liver genes for putative CXCR1, IL 13 receptor alpha 2 (IL13RA2), which is a specific IL-13 receptor, and CD3 glycoprotein (CD3), which increases T cell activation and signaling of humoral immunity [31]. But, STAT2 was down-regulated.

Table 2. Genes identified as differentially expressed due to MOS in non-challenged control hosts1.

MOS increased glucose mobilization and metabolism in non-challenged control chickens

Augmentation in immune responses by MOS among non-challenged control hosts significantly increased glucose mobilization and metabolism. MOS down-regulated the gene for heat shock protein 1 (HSPE1), which folds and activates newly synthesized linear proteins into functional 3-D proteins [32]; thus, deactivated proteins were increasingly utilized in intestinal gluconeogenesis as mediated by PEPCK up-regulation (Table 2). Increased intestinal contractions, in part due to increased glucose absorption across epithelial cells, were mediated by MYH7 up-regulation but not MYH11 and MYL9. Correspondingly, NPPA was up-regulated to ascertain high glucose flux into the liver via the hepatic portal vein. Therefore, to increase the glucose-uptake capacity of liver cells, MOS induced the gene for deiodinase type 2 (DIO2), reported to reduce insulin resistance by increasing intracellular triiodothyronine (T3) levels [33]. Furthermore, down-regulation of potassium voltage-gated channel shaker-related subfamily 3 (KCNA3) significantly increased insulin-stimulated glucose uptake through the GLUT4 glucose transporter, as reported by [34]. As evidenced by ENO2 up-regulation, high liver glucose increased liver glycolytic activities for energy generation. ME and EHHADH down-regulations repressed liver fatty acid biosynthesis and β-oxidation, respectively. Therefore, elevated intestinal gluconeogenesis and liver glycolysis were sufficient to meet the host's energy demands.

LPS mediated innate immune responses differently within MOS and antibiotic chicken groups

So far, we reported inherent immune-stimulatory effects due to independent LPS and MOS treatments. Therefore, simultaneous administration of these treatments was expected to intensify the inflammatory responses. Interestingly, however, our results revealed that MOS counteracted the detrimental effects of LPS on innate immunity. Although we observed intestinal down-regulation of the gene for IL-10, an anti-inflammatory cytokine that causes negative-feedback on secretions of pro-inflammatory cytokines [35], neither IL-3, as observed due to LPS (Table 1) treatment alone, nor any other pro-inflammatory cytokines were induced (Table 3). To further support MOS's effect in alleviating inflammatory responses, we observed down-regulations of TLR2-2, TLR-3 and OAS*A, and IL13RA2 and CD3 in intestinal and liver tissues, respectively. In MOS-fed hosts, innate immune responses after LPS challenge were principally mediated by ZC3H15 down-regulation that enhanced macrophage activation. In VIRG hosts, however, intestinal IL-3 and TLR-3 up-regulations (Table 4) revealed higher LPS-induced inflammatory responses.

Table 3. Genes identified as differentially expressed due to LPS within MOS-fed hosts1.

Table 4. Genes identified as differentially expressed due to LPS within antibiotic-fed hosts1.

LPS mobilized energy differently within MOS and antibiotic chicken groups

To further evidence that MOS reduced innate immune responses, here we report that LPS failed to induce gluconeogenesis or any other major nutrient mobilization processes among MOS-fed hosts (Table 3). Previously, however, we observed increased intestinal gluconeogenesis due to LPS in the absence of MOS (Table 1). These results, together with reduced liver glucose uptake mediated by DIO2 down-regulation and KCNA3 up-regulation, led us to believe that liver glucose levels were sufficiently high to meet the host's energy demands. However, reduced glycolytic activities, due to ENO2 down-regulation, demonstrated that liver glucose levels were abnormally low. Intriguingly, despite reduced glycolysis, we observed up-regulation of the gene for ATP citrate synthase (CS), which catalyzes citrate synthesis from acetyl Co-A and oxaloactetate. Given that citrate is the key regulatory substrate of the TCA cycle, our results indicated that host's energy demands were likely met mainly via the TCA cycle. We also observed that glucose utilization for energy caused down-regulation of UDP glucose pyrophosphorylase 2 (UGP2), which reduces liver glycogen synthesis [36], whereas PRKAG2 up-regulation repressed fatty acid and cholesterol biosynthesis. Finally, MOS down-regulated the gene for α-actin 2 in intestinal smooth muscles (ACTA2) that reduced intestinal contractions [37], whereas MYH11 and MYL9 were up-regulated. Down-regulation of HMGCR repressed intestinal cholesterol synthesis.

Contradictorily, despite VIRG supplementation, LPS challenge profoundly increased gluconeogenesis, as indicated by PEPCK up-regulation in the intestines (Table 4). Evidently, MYH7 was up-regulated whereas ENO2 and HMGCR were down-regulated to suppress intestinal glycolysis and cholesterol synthesis, respectively. But, high glucose influx into the liver increased glycolytic activities through ENO2 up-regulation. Therefore, glucose metabolites were most increasingly utilized in TCA cycle for energy generation. Surprisingly, CS was down-regulated and citrate was instead utilized in fatty acid biosynthesis, as demonstrated by increased expressions of genes for ATP citrate lyase (ACLY), which catalyzes citrate cleavage into acetyl Co-A and oxaloacetate [38], [39], ME and fatty acid synthetase (FAS; as shown in Figure 1A). PFKM down-regulation and NPPA up-regulation occurred in muscle tissues of both MOS- and VIRG-fed hosts.

Figure 1. RT-qPCR validation of microarray data.

LPS up-regulated liver ACLY, ME and FAS among VIRG-fed hosts (A). But, LPS down-regulated these genes in MOS- than VIRG-fed host (B). Intestinal PEPCK was up-regulated among control hosts fed MOS (C), and by LPS among VIRG-fed hosts (D). Data are presented as mean ± SEM (n = 6). *, P<0.01 by Scheffe's t test.

MOS increased innate immune responses in LPS-challenged chickens

In comparisons to LPS-challenged hosts fed VIRG, the additive immune stimulatory effects of LPS and MOS significantly increased innate immune responses as demonstrated by intestinal IL-3 up-regulation, and down-regulation of IL-10 and ZC3H15 (Table 5). But, TLR-3, the corresponding receptor to IL-3, was repressed in the intestines. STAT2 was up-regulated in the liver.

Table 5. Genes identified as differentially expressed due to LPS between MOS- and antibiotic-fed hosts1.

MOS mobilized energy differently than antibiotic in LPS-challenged chickens

Despite increased immune responses in LPS-challenged hosts fed MOS, these chickens faced no detrimental nutrient mobilization processes when compared to LPS-injected hosts fed VIRG. Intestinal gluconeogenesis did not occur although newly-synthesized proteins were deactivated by HSPE1 down-regulation (Table 5). Again, our results about CS up-regulation demonstrate that energy was essentially derived from increasingly synthesized citrate in the liver. Under the effects of LPS, MOS repressed glycogen synthesis by down-regulating UGP2; glycolysis by down-regulating ENO2; fatty acids biosynthesis by down-regulating ACLY, ME and FAS (Table 5 and Figure 1B); and cholesterol biosynthesis by up-regulating PRKAG2. Liver KCNA3 was up-regulated in the absence of high glucose influx. Indeed, these findings are very similar to those observed when comparing MOS-fed hosts in the LPS-challenged and non-challenged control groups.

Real-time quantitative PCR and liver metabolite measurements

To confirm our microarray data, we performed quantitative RT-qPCR analysis on three differentially expressed genes, and measured concentrations of specific liver metabolites. Figure 1 and Tables 2, 4 and 5 show that PEPCK, ACLY and ME expression patterns correlated strongly with microarray results. Moreover liver citrate and pyruvate levels were in agreement with gene expression results (Figure 2). FAS, not present on the array utilized in this study, expression (Figure 1) was determined by RT-qPCR. All RT-qPCR efficiency (E) values were in between 93 to 100%.

Figure 2. Concentrations of liver metabolites.

Among VIRG-fed hosts, LPS reduced liver citrate, but increased pyruvate levels (A). However, higher citrate and lower pyruvate levels were observed in liver of LPS-challenged hosts fed MOS than VIRG (B). Data are presented as mean ± SEM (n = 6). *, P<0.05, **, P<0.01 by Scheffe's t test.


Molecular events underlying late inflammation and subsequently nutrient mobilization, in response to pathogens or antigens, are still not clear. Interestingly, at 24 h post-LPS challenge, microarray results revealed that innate immune responses were principally mediated by IL-3, a pro-inflammatory cytokine that has received little scientific investigations, together with other innate immune mediators (Table 1). Few studies reported IL-3 as playing key roles in linking innate and adaptive immunity. IL-3 is critical for the differentiation of monocytes into dendritic cells, and contributes in proliferation and survival of dendritic cells [40]; dendritic cells are involved in Th cell response. While IL-1 and IL-6 were consistently up-regulated during intense inflammatory responses in poultry [41] and mice [42], here we report that these pro-inflammatory cytokines were not differentially expressed during late inflammation. These results evidenced that inflammation is a time-dependent biological immune reaction, regulated by different immune mediators. Most interestingly, our results revealed that dietary MOS modulated innate immune responses and nutrient metabolisms differently than VIRG.

Our finding that MOS increased immune responses of non-challenged control hosts, but here principally mediated by intestinal IL-3, is consistent with published data [43]-[45], thereby revealing its inherent immune-stimulatory properties. Although the mechanism by which MOS inherently stimulates immunity is unclear, it may be associated with the antigenic properties of yeast cell walls. In contrast, VIRG did not confer such immune stimulatory effects because antibiotics lack antigenic properties. During immune stimulation, an energy-demanding biological process, and the consequential reduction in feed intake, the host's metabolic activities were coordinately regulated to increase energy availability for metabolism. Liver gluconeogenesis, involving muscle catabolism, usually occurs during intense inflammation and starvation [12]. However, here, we observed that gluconeogenesis occurred only in the intestines. Additionally, during the process of glucose synthesis, the preferential utilization of amino acids from ingested feed spared skeletal muscle catabolism. Glucose, mobilized to the liver, was then rapidly metabolized via increased glycolytic activities to meet host's elevated energy demands during the inflammatory response (summarized in Figure 3). Nevertheless, as previously reported [6], [46], MOS's immune-stimulatory effects did not profoundly mobilize glucose and had no detrimental effects on feed intake or growth.

Figure 3. Schematic illustration of the effects of MOS versus VIRG on glucose metabolism in control hosts.

(i) MOS increased intestinal gluconeogenesis by up-regulating PEPCK; (ii) the high glucose influx into the liver was rapidly metabolized by glycolysis as mediated by ENO2 up-regulation; (iii) TCA-derived energy from glycolytic substrates, down-regulated ME and EHHADH which reduced fatty acid synthesis and β-oxidation, respectively.

Both LPS and MOS triggered elevated innate immune responses and glucose mobilization. However, our results that none of the pro-inflammatory cytokines were up-regulated due to continual MOS intake followed by LPS challenge (Tables 3 and S1, S2, S3) revealed that MOS counteracted LPS's detrimental effects on immunity. We also observed that energy demands of hosts fed MOS were sufficiently met by increased TCA cycle-derived energy. Contrastingly, VIRG failed to counteract or reduce LPS's inflammatory effects, as indicated by increased IL-3 expression (Table 4). The higher energy demands of VIRG hosts necessitated glucose mobilization through intestinal gluconeogenesis and increased liver glycolytic activities. Based on these findings, we conclude that dietary MOS helped terminate LPS-induced inflammation earlier than VIRG. This beneficial effect of MOS may be explained by its inherent immune-stimulatory properties that caused mild immune stimulation, thereby ‘arming’ the body's defense mechanisms to rapidly and efficiently clear the endotoxin.

However, increased TCA activities surprisingly occurred among hosts fed MOS despite their reduced glycolytic activities. Although fatty acid and cholesterol synthesis genes are coordinately down-regulated during LPS-triggered systemic inflammation [47], we observed increased liver de novo fatty acid synthesis among hosts fed VIRG despite increased intestinal gluconeogenesis and liver glycolysis. Generally, fatty acid synthesis, which converts excess energy into energy reserves, occurs only when dietary carbohydrate intake exceeds immediate energy requirements. But, we observed a reduction in feed intake due to LPS challenge. Because inflammation is a dynamic biological immune reaction, molecular events at 24 h post-LPS challenge are a consequence of earlier immunological events. To help explain these apparently conflicting observations, we will briefly consider nutrient mobilization during intense inflammation. Whereas glycogenolysis and gluconeogenesis are frequently reported during intense inflammation, significant mobilization and catabolism of glucose may have significantly increased liver glucose and its glucose metabolites, including acetyl Co-A, pyruvate and citrate, levels in both MOS- and VIRG-fed hosts. In the absence of innate immune responses at 24 h post-LPS challenge, increased activity of CS, a key enzyme involved in TCA cycle, revealed that energy demands of MOS-fed hosts were mainly derived from liver glucose/glucose metabolites that accumulated earlier. Evidently, intestinal gluconeogenesis and liver glycolysis were not necessary and repressed (summarized in Figure 4).

Figure 4. Schematic illustration of MOS effects on glucose metabolism between control and LPS-challenged hosts.

(i) LPS triggered no major intestinal metabolic activities; (ii) in absence of glucose mobilization, liver glucose uptake and transport were repressed by DIO2 down-regulation and KCNA3 up-regulation, respectively; (iii) glycolysis and glycogen synthesis were coordinately reduced by ENO2 and UGP2 down-regulation, respectively; (iv) CS up-regulation increased TCA-derived energy from high liver pyruvate; (v) PRKAG2 up-regulation inhibited fatty acid and cholesterol biosynthesis.

In VIRG-fed hosts, however, elevated innate immune responses at 24 h post-LPS challenge required higher energy. Insufficient energy derived from accumulated liver glucose/glucose metabolites necessitated further glucose mobilization and catabolism through intestinal gluconeogenesis and liver glycolysis, respectively. However, as evidenced by ACLY up-regulation, exceptionally high liver citrate levels, which accumulated during intense inflammation, triggered CS down-regulation. Citrate is well recognized as a potent allosteric negative-feedback inhibitor of CS activity and plays a crucial role in liver metabolic activities. Evidently, to rapidly catabolize and deplete the accumulated liver cytosolic citrate after its efflux from the mitochondria where it is synthesized, (i) ACLY up-regulation generated high acetyl Co-A levels, (ii) ME up-regulation increased liver NADPH concentrations, (iii) whereas FAS up-regulation synthesized palmitate, the major fatty acid that ultimately yields long fatty acid chains, from acetyl Co-A, NADPH and malonyl Co-A, which is synthesized from acetyl Co-A by acetyl Co-A carboxylase (summarized in Figure 5). ACLY, ME and FAS are key lipogenic enzymes that convert liver cytoplasmic citrate into fatty acids. The preferential acetyl Co-A and NADPH utilization in de novo fatty acid biosynthesis mediated by ACLY, ME and FAS up-regulations is consistent with published reports [48]. In previously fasted and refed rats and chickens, increased liver lipogenesis was also mediated by ACLY, ME and FAS up-regulations [49], [50]. While increased glucose mobilization and decreased fatty acid synthesis have frequently been reported during intense inflammation [47], [51], here we report that the liver rapidly metabolized citrate into fatty acids to restore its citrate homoeostatic level during late inflammation in addition to glucose mobilization for body energy requirements.

Figure 5. Schematic illustration of VIRG effects on glucose metabolism between control and LPS-challenged hosts.

(i) LPS increased intestinal gluconeogenesis by up-regulating PEPCK; (ii) mobilized glucose increased liver glycolytic activities through ENO2 up-regulation; (iii) CS down-regulation reduced utilization of glycolytic substrates by the TCA cycle for energy; (iv) ACLY, ME and FAS up-regulations increased liver fatty acid biosynthesis from high liver citrate.

In agreement with O'Hea and Leveille [52], we observed that livers in chickens derived most of the NADPH required for fatty acid synthesis from the ME reaction, whereas livers in rats obtained about 65% of NADPH from the pentose phosphate pathway [53]. Collectively, these findings indicate that significantly more glucose was mobilized from the intestine and more glucose metabolites accumulated in the liver of VIRG hosts during the period of intense inflammation than MOS-fed hosts, and that VIRG failed to terminate innate immune responses earlier. But, when challenged with LPS, we observed an elevation in innate immune responses, principally mediated by intestinal IL-3, among hosts fed MOS than VIRG. Although these results were not surprising considering the additive immune-stimulatory effects of MOS and LPS, no major nutrient mobilization processes occurred among LPS-challenged hosts fed MOS (summarized in Figure 6). TCA-derived energy from high liver glucose and glucose metabolites which accumulated earlier than 24 h of LPS challenge was sufficient to meet energy demands of the hosts fed MOS.

Figure 6. Schematic illustration of LPS effects on glucose metabolism between MOS- and VIRG-fed hosts.

(i) LPS caused no major intestinal metabolic activities in MOS-fed hosts; (ii) in absence of liver glucose mobilization, KCNA3 was up-regulated, whereas ENO2 and UGP2 down-regulation reduced glycolysis and glycogen synthesis, respectively; (iii) CS up-regulation increased TCA cycle-derived energy from high liver pyruvate; (iv) ACLY, ME and FAS down-regulations inhibited liver fatty acid biosynthesis; whereas PRKAG2 up-regulation inhibited fatty acid and cholesterol biosynthesis.

Livers and kidneys are well-recognized gluconeogenic organs in humans and mice [54], [55]. Whereas the intestine is equivocally reported as a gluconeogenic organ in mice [56], [57], we are among the first to demonstrate that the chicken small intestine, but not skeletal muscles, is also a gluconeogenic organ that was regulated by PEPCK. We have discussed the increased intestinal gluconeogenesis at 24 h post-LPS challenge. Given that MOS and VIRG are not absorbed across the intestinal epithelium, these macromolecules produce localized effects in the intestines. Therefore, all our findings evidenced cross talks between intestinal mucosal immunity and systemic immunity. This is the first study demonstrating that MOS can beneficially modulate innate immunity and nutrient metabolism during late systemic inflammation.

In summary, late inflammation was principally modulated by IL-3. In contrast to antibiotics like VIRG, MOS elicited several beneficial responses: (i) terminated Salmonella LPS-induced systemic inflammation earlier, presumably due to its inherent intestinal innate immune-stimulatory properties; and (ii) reduced the magnitude of glucose mobilization. Therefore, this study potentiates the use of natural immuno-modulators, such as a MOS, to attenuate Salmonella-induced systemic inflammation both among human and animal hosts, and without posing the risk of antibiotic-resistance development.

Materials and Methods

Chickens, experimental diets and LPS challenge

Hatched chicks (Cobb 500 broilers) were raised in two groups (n = 64/group). In each bird group (8 cages/diet), half was fed a diet containing MOS (2 kg/ton BioMos®; Alltech Inc., Nicholasville, KY) or virginiamycin (16.5 mg/kg), as described [46]. To induce an acute inflammatory response, group 1 hosts (n = 64) were injected i.p. with 3 ml of Salmonella Typhimurium LPS (100 mg LPS/L, Sigma-Aldrich, ON, Canada) whereas group 2 control hosts were saline-injected at 14 d of age. All animal procedures were approved by the McGill Animal Care Committee (protocol number 5399). All hosts had free access to feed and water.

Bodyweight, feed intake and body temperature measurements

All non-challenged control (saline-injected) and LPS-challenged hosts were individually weighed at 0 (initial BW), 12, 24 and 48 h post-injection to determine BW gain relative to initial BW. Average feed consumption of chickens was calculated at similar time points. Body temperatures were recorded after 0, 2, 4, 6, 8, 12, 24 and 48 h of saline or LPS injection using a thermocouple rectal probe thermometer (Physitemp Instruments Inc., Clifton, NJ).

Liver weights and tissue samples collection

Chickens (n = 8/diet/group) were randomly euthanized at 12, 24 and 48 h post-injection and liver weights of respective chickens were expressed relative to their final BW. At 24 h after saline and LPS injections, liver, intestine (jejunum) and skeletal muscle (breast meat) samples (n = 6 /diet/group) were immediately snap frozen in liquid nitrogen, and stored at −80°C for later RNA extraction.

Microarray analysis

After 24 h, total RNA was extracted from liver, intestine (jejunum) and skeletal muscle (breast) tissues using Trizol reagent and Purelink RNA Mini Kit (Invitrogen). Isolated total RNA was quantified on the basis of its absorption at 260 nm using a Nanodrop® ND-1000 spectrophotometer (NanoDrop Technologies, Wilmington, DE), and visualized on an agarose gel to check quality. RNA was retrotranscribed into Cy3 or Cy5 aminoallyl labelled cDNA and hybridized onto chicken-specific focused oligonucleotides microarrays. The microarray platform used (accession number GPL13457) and data files (accession number GSE28959) are registered at the MIAME compliant National Centre for Biotechnology Information (NCBI) Gene Expression Omnibus (GEO) archive ( Briefly, 70mers chicken-specific oligonucleotides, obtained from Operon Biotechnologies Inc. (Germantown, MD), were spot printed on UltraGAPS Amino-Silane Coated Slides (Corning Inc., Acton, MA) as described [58]. Each oligonucleotide sequence (probe) was replicated 12 times per array.

cDNA labeling and microarray hybridization

A total of 12 microarrays was used per tissue and chicken group (n = 6/diet) in a 2×2 factorial design and complete interwoven loop arrangement (Figure S5; [59]). First, RNA was retrotranscribed into aminoallyl labelled cDNA using the ChipShot Indirect Labelling and Clean-Up System Kit (Promega, Madison, WI) and Cy3 or Cy5 fluorescent dye (Amersham Biosciences Corp., Piscataway, NJ) according to the manufacturer's recommendations. Reverse transcription was carried out at 42°C for 2 h, followed by RNase H digestion for 15 min at 37°C. Briefly, a reactive amine derivative of 5-(3-aminoallyl)-2′-deoxyuridine 5′-triphosphate was incorporated during reverse transcription. Subsequent to reverse transcriptase reaction, succinimidyl esters of Cy3 or Cy5 were covalently bonded to aminoallyl-labelled cDNAs. Cy-3 and Cy-5 labelled cDNA were then purified, combined and hybridized to the array for 24 h in darkness by making use of the Pronto Plus! Microarray Hybridisation Kit (Corning Inc., NY).

Microarray data analysis

Hybridized arrays were scanned twice at 65% (Cy3) and 50% (Cy5) laser power using a ScanArray GX PLUS Microarray Scanner (PerkinElmer Life and Analytical Sciences, Shelton, CT) to obtain Cy3∶Cy5 intensity ratios of labelled cDNA hybridized to complementary oligonucleotide sequences on the array. Spot intensity data were extracted using the ScanAlyze Software (Standford University, Standford, CA) and analyzed using the JMP Genomics software (SAS Institute Inc., Cary, NC). Data were log2 transformed prior to normalization by using locally weighted regression and smoothing, first within array (ratio analysis) and then across arrays (Lowess normalization). Normalized data were monitored by distribution analysis of the transformed data. Finally, the normalized log2 transformed data were analyzed using a two-way ANOVA, as described [60]. Expression values were modeled as: Yijklm = μ+Ai+Cj+Dk+Il+DIkl+eijklm, where μ represents the overall mean value, Ai: random effect for arrays (i = 1, 2…‥12), Cj: main effect of Cy-dye (j = Cy-3 or Cy-5), Dk: main effect of diet (k = MOS or VIRG), Il: main effect of injection (l = saline or LPS), and DIkl: interaction effect between diet and injection, and eijklm: random error. Mean intensities were tested using the false discovery rate (FDR) multiple comparison t test and differentially expressed genes were declared at P<0.05. Finally, for each pairwise comparison, significantly different genes were filtered based on their mean intensity values to determine up- or down-regulated genes due to diet, injection and diet*injection.

Real-time quantitative PCR analysis

Real-time quantitative PCR (RT-qPCR) was used for validation of differential gene expressions observed in microarrays. Total RNA was retrotranscribed into cDNA by using 1 µg total RNA and iScript cDNA Synthesis Kit (Bio-Rad, ON, Canada), following the manufacturer's instructions. RT-qPCR was performed using the Bio-Rad CFX384 RT-qPCR Detection System, SsoFast Evagreen Supermix (Bio-Rad) and primer-set sequences (Table 6). RT-qPCR reactions were performed at 95°C for 5 min, followed by 39 cycles of 95°C for 15 s and 60°C for 30 s. A melting curve program was included at the end of each RT-qPCR to verify presence of a unique product. Relative intestinal (PEPCK) and liver (ACLY, ME, CS and FAS) gene expression levels were normalized to GAPDH or beta-2 microglobulin, respectively. The expression stability of the reference genes were tested using the geNorm software (available at: Samples were analyzed in technical duplicates, and differential gene expressions were determined using the comparative standard curve method.

Table 6. Primers-set sequences used to analyze gene expression by quantitative PCR.

Liver metabolites measurements

Liver citrate and pyruvate levels were measured by specific enzymatic reactions using the Citrate and Pyruvate Assay Kits (BioVision, CA, USA), following the manufacturer's instructions with few modifications. Briefly, 0.5 g of liver tissues were homogenized completely by sonication in 700 µL of respective buffer solutions and then centrifuged at 15,000 g for 10 mins to remove cell debris. After the supernatant was deproteinized using the Deproteinizing Sample Preparation Kit (BioVision), a 100 µL sample volume was used for analysis. Reaction mix was prepared without buffer dilution.

Statistical analysis

Except for microarray data, all data were analyzed as a two-way ANOVA and a 2×2 factorial arrangement to determine the main effects of diet and injection, and their interaction effects by using the MIXED procedure of SAS (SAS Institute, 2003). For bodyweight, liver weight and body temperature data, a Nested Model Design was also employed with cages nested within diet*injection, as follows: Yijkl = μ+Dieti+Injectionj+Dieti*Injectionj+Cageijk+eijkl, where μ represents the overall mean value, Dieti: fixed effect of diet (i = MOS or VIRG), Injectionj: fixed effect of injection (j = saline or LPS), Dieti * Injectionj: interaction effect between diet and injection, Cageijk: random effect of cage nested within diet*injection (k = 1,2,…8), and eijkl: random error. Differences among treatment means were tested using Scheffe's t test and statistical significance declared at P<0.05.

Supporting Information

Figure S1.

Innate immune-stimulatory effects of LPS caused elevation in body temperatures. Antibiotic (VIRG)- and MOS-fed hosts were injected i.p. with LPS. At 0, 2 and 48 h after injection, body temperatures were not different between LPS-challenged and non-challenged control (saline) hosts (A), or between VIRG- and MOS-fed hosts within the LPS-challenged or control group, respectively (B), or between hosts fed VIRG and MOS (C). However, in comparison with control hosts, LPS significantly increased (P<0.05) body temperatures at 4, 6, 8, 12 and 24 h post-injection (A). But, such increase in body temperatures were not observed between VIRG and MOS hosts within the LPS-challenged or control group, respectively (B), or between VIRG- and MOS-fed hosts irrespective of injection type (C). Results are expressed as mean ± SEM. Supercripts: (a,b) denote statistical differences among treatment means at a particular time point, P<0.05, Scheffe's multi-comparison t-test.


Figure S2.

The effects of LPS injected i.p. on feed intake in antibiotic- (VIRG) and MOS-fed hosts. LPS significantly reduced feed intake (P<0.05) at 12 h post-injection (A). However, feed intake was not different between hosts fed the VIRG and MOS diet (B), or between VIRG and MOS hosts within the LPS-challenged or non-challenged control (saline) group, respectively (C). At 24 and 48 h post-injection, feed intake was not different between LPS and control hosts (A), hosts fed the VIRG and MOS diet (B), or between VIRG and MOS hosts within the LPS-challenged or control group, respectively (C). Results are expressed as mean ± SEM. Supercripts: (a,b) denote statistical differences among treatment means at a particular time, P<0.05, Scheffe's multi-comparison t-test.


Figure S3.

The effects of LPS injected i.p. on bodyweight (BW) gain in antibiotic- (VIRG) and MOS fed hosts. LPS significantly reduced BW (P<0.05) after 12, 24 and 48 h of injection (A). In contrast to MOS-fed hosts, those fed VIRG grew faster (P<0.05) at 48 h only (B). But, BW gain was not different between VIRG and MOS hosts within the LPS-challenged or non-challenged control (saline) group, respectively (C). Results are expressed as mean ± SEM. Supercripts: (a,b) denote statistical differences among treatment means at a particular time point, P<0.05, Scheffe's multi-comparison t-test.


Figure S4.

The effects of LPS injected i.p. on liver weights of antibiotic- (VIRG) and MOS fed hosts. LPS significantly increased (P<0.05) liver weights at 12 and 24 h post-injection, but not after 48 h (A). However, at all times, liver weights were not different between hosts fed the VIRG and MOS diet (B), or between VIRG and MOS hosts within the LPS-challenged or non-challenged control (saline) group, respectively (C). Results are expressed as mean ± SEM. Supercripts: (a,b) denote statistical differences among treatment means at a particular time, P<0.05, Scheffe's multi-comparison t-test.


Figure S5.

Schematic of the 2×2 factorial experimental design in an interwoven loop arrangement for each tissue (liver, intestine or skeletal muscles). Diet×Injection is denoted as VC (VIRG×non-challenged control hosts), VL (VIRG×LPS-challenged hosts), BC (MOS×non-challenged control hosts), and BL (MOS×LPS-challenged hosts). Each arrow represents an array (total: 12) consisting of 2 aminoallyl labelled cDNA, either Cy-3 or Cy-5.


Table S1.

Fold change and P values of gene expressions due to prebiotic and antibiotic in intestinal tissues of non-challenged control and LPS-challenged birds.


Table S2.

Fold change and P values of gene expressions due to prebiotic and antibiotic in liver tissues of non-challenged control and LPS-challenged birds.


Table S3.

Fold change and P values of gene expressions due to prebiotic and antibiotic in skeletal muscle tissues of non-challenged control and LPS-challenged birds.


Author Contributions

Conceived and designed the experiments: BB PF XZ. Performed the experiments: BB. Analyzed the data: BB JdO. Contributed reagents/materials/analysis tools: BB CMA. Wrote the paper: BB. Reviewed manuscript: XZ PF.


  1. 1. CDC (2011) Salmonella Serotype Enteritidis. Available at: nczved/divisions/dfbmd /diseases/salmonella_enteritidis/ Accessed: July 1, 2011.
  2. 2. Griffin AJ, McSorley SJ (2011) Development of protective immunity to Salmonella, a mucosal pathogen with a systemic agenda. Mucosal Immunol 4: 371–382.
  3. 3. Zhao C, Ge B, De Villena J, Sudler R, Yeh E, et al. (2001) Prevalence of Campylobacter spp., Escherichia coli, and Salmonella serovars in retail chicken, turkey, pork, and beef from the Greater Washington, D.C., area. Appl Environ Microbiol 67: 5431–5436.
  4. 4. WHO (2011) Complacency kills. Antibiotic resistance still on the rise in Europe. WHO raises the alert on World Health Day. World Health Organization website (accessed 2011 Oct 3). Available:
  5. 5. Ofek I, Beachey EH (1978) Mannose binding and epithelial cell adherence of Escherichia coli. Infect Immun 22: 247–254.
  6. 6. Baurhoo B, Letellier A, Zhao X, Ruiz-Feria CA (2007) Cecal populations of lactobacilli and bifidobacteria and Escherichia coli populations after in vivo Escherichia coli challenge in birds fed diets with purified lignin or mannanoligosaccharides. Poult Sci 86: 2509–2516.
  7. 7. Hoshino K, Takeuchi O, Kawai T, Sanjo H, Ogawa T, et al. (1999) Cutting edge: Toll-like receptor 4 (TLR4)-deficient mice are hyporesponsive to lipopolysaccharide: evidence for TLR4 as the Lps gene product. J Immunol 162: 3749–3752.
  8. 8. Akira S, Uematsu S, Takeuchi O (2006) Pathogen recognition and innate immunity. Cell 124: 783–801.
  9. 9. Xie H, Rath NC, Huff GR, Huff WE, Balog JM (2000) Effects of Salmonella Typhimurium lipopolysaccharide on broiler chickens. Poult Sci 79: 33–40.
  10. 10. Harden LM, du Plessis I, Poole S, Laburn HP (2008) Interleukin (IL)-6 and IL-1 beta act synergistically within the brain to induce sickness behavior and fever in rats. Brain Behav Immun 22: 838–849.
  11. 11. Doyle A, Zhang GH, Fattah EAA, Eissa NT, Li YP (2011) Toll-like receptor 4 mediates lipopolysaccharide-induced muscle catabolism via coordinate activation of ubiquitin-proteasome and autophagy-lysosome pathways. FASEB J 25: 99–110.
  12. 12. Flores EA, Bistrian BR, Pomposelli JJ, Dinarello CA, Blackburn GL, et al. (1989) Infusion of tumor necrosis factor/cachectin promotes muscle catabolism in the rat. A synergistic effect with interleukin 1. J Clin Invest 83: 1614–1622.
  13. 13. Holecek M, Skopec F, Sprongl L, Pecka M (1995) Protein metabolism in specific tissues of endotoxin-treated rats: effect of nutritional status. Physiol Res 44: 399–406.
  14. 14. Feingold KR, Staprans I, Memon RA, Moser AH, Shigenaga JK, et al. (1992) Endotoxin rapidly induces changes in lipid metabolism that produce hypertriglyceridemia: low doses stimulate hepatic triglyceride production while high doses inhibit clearance. J Lipid Res 33: 1765–1776.
  15. 15. Cook DN, Pisetsky DS, Schwartz DA (2004) Toll-like receptors in the pathogenesis of human disease. Nat Immunol 5: 975–979.
  16. 16. Clarke TB, Davis KM, Lysenko ES, Zhou AY, Yu Y, et al. (2011) Recognition of peptidoglycan from the microbiota by Nod1 enhances systemic innate immunity. Nat Med 16: 228–231.
  17. 17. Galdeano CM, Nunez IN, de LeBlanc AD, Carmuega E, Weill R, et al. (2011) Impact of a probiotic fermented milk in the gut ecosystem and in the systemic immunity using a non-severe protein-energy-malnutrition model in mice. BMC Gastroenterology 11: 64.
  18. 18. Stern CD (2005) The chick; a great model system becomes even greater. Dev Cell 8: 9–17.
  19. 19. Lopez-Bojorquez LN, Dehesa AZ, Reyes-Teran G (2004) Molecular mechanisms involved in the pathogenesis of septic shock. Arch Med Res 35: 465–479.
  20. 20. Liang J, Song W, Tromp G, Kolattukudy PE, Fu M (2008) Genome-wide survey and expression profiling of CCCH-zinc finger family reveals a functional module in macrophage activation. PLoS One 3: e2880.
  21. 21. Decker T, Stockinger S, Karaghiosoff M, Muller M, Kovarik P (2002) IFNs and STATs in innate immunity to microorganisms. J Clin Invest 109: 1271–1277.
  22. 22. Kirschning CJ, Wesche H, Merrill Ayres T, Rothe M (1998) Human toll-like receptor 2 confers responsiveness to bacterial lipopolysaccharide. J Exp Med 188: 2091–2097.
  23. 23. Hasenstein JR, Lamont SJ (2007) Chicken gallinacin gene cluster associated with Salmonella response in advanced intercross line. Avian Dis 51: 561–567.
  24. 24. Behera AK, Kumar M, Lockey RF, Mohapatra SS (2002) 2′–5′ Oligoadenylate synthetase plays a critical role in interferon-gamma inhibition of respiratory syncytial virus infection of human epithelial cells. J Biol Chem 277: 25601–25608.
  25. 25. Goldstein JL, Brown MS (1990) Regulation of the mevalonate pathway. Nature 343: 425–430.
  26. 26. van Rooij E, Quiat D, Johnson BA, Sutherland LB, Qi XX, et al. (2009) A family of microRNAs encoded by myosin genes governs myosin expression and muscle performance. Dev Cell 17: 662–673.
  27. 27. Hillgartner FB, Charron T (1998) Glucose stimulates transcription of fatty acid synthase and malic enzyme in avian hepatocytes. Am J Physiol 274: E493–501.
  28. 28. Waterson RM, Hill RL (1972) Enoyl coenzyme A hydratase (crotonase). Catalytic properties of crotonase and its possible regulatory role in fatty acid oxidation. J Biol Chem 247: 5258–5265.
  29. 29. Hardie DG (2003) Minireview: the AMP-activated protein kinase cascade: the key sensor of cellular energy status. Endocrinology 144: 5179–5183.
  30. 30. Nsenga R, Cheng L, Mei'an HE, Tangchun WU (2009) The role of natriuretic peptide precursor A gene polymorphism in the development of coronary heart disease in Chinese Han population. Front Med China 3: 437–442.
  31. 31. Letourneur F, Klausner RD (1992) Activation of T cells by a tyrosine kinase activation domain in the cytoplasmic tail of CD3 epsilon. Science 255: 79–82.
  32. 32. Ostermann J, Horwich AL, Neupert W, Hartl FU (1989) Protein folding in mitochondria requires complex formation with hsp60 and ATP hydrolysis. Nature 341: 125–130.
  33. 33. Chidakel A, Mentuccia D, Celi FS (2005) Peripheral metabolism of thyroid hormone and glucose homeostasis. Thyroid 15: 899–903.
  34. 34. Xu J, Wang P, Li Y, Li G, Kaczmarek LK, et al. (2004) The voltage-gated potassium channel Kv1.3 regulates peripheral insulin sensitivity. Proc Natl Acad Sci USA 101: 3112–3117.
  35. 35. Taylor A, Verhagen J, Blaser K, Akdis M, Akdis CA (2006) Mechanisms of immune suppression by interleukin-10 and transforming growth factor-beta: the role of T regulatory cells. Immunology 117: 433–442.
  36. 36. Ferrer JC, Favre C, Gomis RR, Fernandez-Novell JM, Garcia-Rocha M, et al. (2003) Control of glycogen deposition. FEBS Lett 546: 127–132.
  37. 37. Guo DC, Pannu H, Tran-Fadulu V, Papke CL, Yu RK, et al. (2007) Mutations in smooth muscle alpha-actin (ACTA2) lead to thoracic aortic aneurysms and dissections. Nat Genet 39: 1488–1493.
  38. 38. Cheema-Dhadli S, Halperin ML, Leznoff CC (1973) Inhibition of enzymes which interact with citrate by (–)hydroxycitrate and 1,2,3,-tricarboxybenzene. Eur J Biochem 38: 98–102.
  39. 39. Pearce NJ, Yates JW, Berkhout TA, Jackson B, Tew D, et al. (1998) The role of ATP citrate-lyase in the metabolic regulation of plasma lipids - Hypolipidaemic effects of SB-204990, a lactone prodrug of the potent ATP citrate-lyase inhibitor SB-201076. Biochemical J 334: 113–119.
  40. 40. Ebner S, Hofer S, Nguyen VA, Furhapter C, Herold M, et al. (2002) A novel role for IL-3: human monocytes cultured in the presence of IL-3 and IL-4 differentiate into dendritic cells that produce less IL-12 and shift Th cell responses toward a Th2 cytokine pattern. J Immunol 168: 6199–6207.
  41. 41. Kogut MH, He H, Kaiser P (2005) Lipopolysaccharide binding protein/CD14/ TLR4-dependent recognition of Salmonella LPS induces the functional activation of chicken heterophils and up-regulation of pro-inflammatory cytokine and chemokine gene expression in these cells. Anim Biotechnol 16: 165–181.
  42. 42. Park EJ, Lee JH, Yu GY, He GB, Ali SR, et al. (2010) Dietary and Genetic Obesity Promote Liver Inflammation and Tumorigenesis by Enhancing IL-6 and TNF Expression. Cell 140: 197–208.
  43. 43. Gao J, Zhang HJ, Yu SH, Wu SG, Yoon I, et al. (2008) Effects of yeast culture in broiler diets on performance and immunomodulatory functions. Poult Sci 87: 1377–1384.
  44. 44. Gomez-Verduzco G, Cortes-Cuevas A, Lopez-Coello C, Avila-Gonzalez E, Nava GM (2009) Dietary supplementation of mannan-oligosaccharide enhances neonatal immune responses in chickens during natural exposure to Eimeria spp. Acta Vet Scand 51: 11.
  45. 45. Szymanska-Czerwinska M, Bednarek D, Zdzisinska B, Kandefer-Szerszen M (2009) Effect of tylosin and prebiotics on the level of cytokines and lymphocyte immunophenotyping parameters in calves. Central Eur J Immunol 34: 1–6.
  46. 46. Baurhoo B, Ferket PR, Zhao X (2009) Effects of diets containing different concentrations of mannanoligosaccharide or antibiotics on growth performance, intestinal development, cecal and litter microbial populations, and carcass parameters of broilers. Poult Sci 88: 2262–2272.
  47. 47. Yoo JY, Desiderio S (2003) Innate and acquired immunity intersect in a global view of the acute-phase response. Proc Natl Acad Sci USA 100: 1157–1162.
  48. 48. Morral N, Edenberg HJ, Witting SR, Altomonte J, Chu T, et al. (2007) Effects of glucose metabolism on the regulation of genes of fatty acid synthesis and triglyceride secretion in the liver. J Lipid Res 48: 1499–1510.
  49. 49. Kochan Z, Karbowska J, Swierczynski J (1997) Unususal increase of lipogenesis in rat white adipose tissue after multiple cycles of starvation-refeeding. Metabolism 46: 10–17.
  50. 50. Wang PH, Ko YH, Chin HJ, Hsu C, Ding ST, et al. (2009) The effect of feed restriction on expression of hepatic lipogenic genes in broiler chickens and the function of SREBP1. Comp Biochem Physiol 153: 327–331.
  51. 51. Ceciliani F, Giordano A, Spagnolo V (2002) The systemic reaction during inflammation: The acute-phase proteins. Protein and Peptide Letters 9: 211–223.
  52. 52. O'Hea EK, Leveille GA (1968) Lipogenesis in Isolated Adipose Tissue of Domestic Chick (Gallus Domesticus). Comp Biochem Physiol 26: 111–120.
  53. 53. Flatt JP, Ball EG (1966) Studies on the metabolism of adipose tissue. XIX. An evaluation of the major pathways of glucose catabolism as influenced by acetate in the presence of insulin. J Biol Chem 241: 2862–2869.
  54. 54. Stumvoll M, Meyer C, Perriello G, Kreider M, Welle S, et al. (1998) Human kidney and liver gluconeogenesis: evidence for organ substrate selectivity. Am J Physiol 274: E817–826.
  55. 55. Eid A, Bodin S, Ferrier B, Delage H, Boghossian M, et al. (2006) Intrinsic gluconeogenesis is enhanced in renal proximal tubules of Zucker diabetic fatty rats. J Am Soc Nephrol 17: 398–405.
  56. 56. Croset M, Rajas F, Zitoun C, Hurot JM, Montano S, et al. (2001) Rat small intestine is an insulin-sensitive gluconeogenic organ. Diabetes 50: 740–746.
  57. 57. Martin G, Ferrier B, Conjard A, Martin M, Nazaret R, et al. (2007) Glutamine gluconeogenesis in the small intestine of 72 h-fasted adult rats is undetectable. Biochem J 401: 465–473.
  58. 58. Druyan S, de Oliveira JE, Ashwell CM (2008) Focused microarrays as a method to evaluate subtle changes in gene expression. Poult Sci 87: 2418–2429.
  59. 59. Garosi P, De Filippo C, van Erk M, Rocca-Serra P, Sansone SA, et al. (2005) Defining best practice for microarray analyses in nutrigenomic studies. Br J Nutr 93: 425–432.
  60. 60. Wolfinger RD, Gibson G, Wolfinger ED, Bennett L, Hamadeh H, et al. (2001) Assessing gene significance from cDNA microarray expression data via mixed models. J Comput Biol 8: 625–637.