Falcarinol Is a Potent Inducer of Heme Oxygenase-1 and Was More Effective than Sulforaphane in Attenuating Intestinal Inflammation at Diet-Achievable Doses

Stefanson, Amanda L.; Bakovic, Marica

doi:https://doi.org/10.1155/2018/3153527

Oxidative Medicine and Cellular Longevity

On this page

Abstract Introduction Methods Results Discussion Data Availability Conflicts of Interest Acknowledgments References Copyright Related Articles

Special Issue

Bioactive Compounds of Food: Their Role in the Prevention and Treatment of Diseases

View this Special Issue

Research Article | Open Access

Volume 2018 | Article ID 3153527 | https://doi.org/10.1155/2018/3153527

Falcarinol Is a Potent Inducer of Heme Oxygenase-1 and Was More Effective than Sulforaphane in Attenuating Intestinal Inflammation at Diet-Achievable Doses

Amanda L. Stefanson¹and Marica Bakovic¹

Guest Editor: Felipe L. de Oliveira

Received11 May 2018

Revised20 Aug 2018

Accepted02 Sept 2018

Published21 Oct 2018

Abstract

Nuclear factor- (erythroid-derived 2) like 2 (Nrf2) is a transcription factor that regulates the expression of a battery of antioxidant, anti-inflammatory, and cytoprotective enzymes including heme oxygenase-1 (Hmox1, Ho-1) and NADPH:quinone oxidoreductase-1 (Nqo1). The isothiocyanate sulforaphane (SF) is widely understood to be the most effective natural activator of the Nrf2 pathway. Falcarinol (FA) is a lesser studied natural compound abundant in medicinal plants as well as dietary plants from the Apiaceae family such as carrot. We evaluated the protective effects of FA and SF (5 mg/kg twice per day in CB57BL/6 mice) pretreatment for one week against acute intestinal and systemic inflammation. The phytochemical pretreatment effectively reduced the magnitude of intestinal proinflammatory gene expression (IL-6, Tnfα/Tnfαr, Infγ, STAT3, and IL-10/IL-10r) with FA showing more potency than SF. FA was also more effective in upregulating Ho-1 at mRNA and protein levels in both the mouse liver and the intestine. FA but not SF attenuated plasma chemokine eotaxin and white blood cell growth factor GM-CSF, which are involved in the recruitment and stabilization of first-responder immune cells. Phytochemicals generally did not attenuate plasma proinflammatory cytokines. Plasma and intestinal lipid peroxidation was also not significantly changed 4 h after LPS injection; however, FA did reduce basal lipid peroxidation in the mesentery. Both phytochemical pretreatments protected against LPS-induced reduction in intestinal barrier integrity, but FA additionally reduced inflammatory cell infiltration even below negative control.

1. Introduction

The gastrointestinal (GI) tract is the largest interface between the body and the environment, followed by the lung and the integument, with ratios of an estimated surface area approximately 150 : 50 : 1. The small intestine is the majority component of the GI tract; its surface was composed of a single monolayer of intestinal epithelial cells which secrete a glycocalyx matrix and a layer of mucous. This delicate barrier performs the diametric roles of digestion and absorption of nutrients and protection against pathogenic microorganisms and innumerable xenobiotic compounds from the environment [1]. In addition, the small intestine is the organ of first pass detoxification [2] and provides the milieu for a large proportion of the immune system [1, 3]. Likely due to this challenging physiological role, small intestinal epithelial cells have the highest turnover rates and are replaced every 2–6 days [4]. It is recognized that chronic and degenerative disease is rooted in early deviations from normal homeostasis that underpin the development of a wide variety of disparate disease pathologies. For example, unresolved inflammation contributes to cardiovascular disease, type 2 diabetes, metabolic syndrome, and neurodegenerative disease to name only a few. Intestinal barrier integrity is a lesser appreciated early deviation from homeostasis that contributes to many intestinal diseases (IBD, IBS, and celiac disease to name a few [5–7]) but also many other widely divergent pathologies. Barrier integrity has been implicated in autoimmune diseases, food allergies, obesity, endotoxemia, and chronic inflammation [5, 8, 9]. In fact, intestinal barrier function is very sensitive to seemingly unrelated traumas such as burn injury [10–12], hemorrhagic shock [13, 14], and even intense exercise [15–19].

Intraperitoneal lipopolysaccharide (LPS) is absorbed in the tissues of the peritoneal space, making its way into systemic circulation, where it is rapidly cleared from the bloodstream (minutes to hours [20, 21]) and slowly (over days [22, 23]) excreted from the organism in bile through liver metabolism, in the urine through kidney filtration, but also through the shedding of epithelial cells at the villus tip in the small intestine. The liver clears two thirds of circulating LPS via sinusoidal endothelial cells and Kuppfer cells [21], which is then secreted into the intestine via the bile [24]; in the lumenal environment of the intestine, there is a high tolerance for LPS due to the constant interaction with gram-negative bacteria in the microbiome [25, 26] and it does not trigger inflammation [27, 28]. LPS is ultimately excreted in feces [29, 30]. Some LPS loses occur via urinary excretion [30]. But another route of excretion is via the small intestine, where LPS appears first in the crypts and then concentrates in the small intestinal epithelial cells of the villus tips [31, 32], which are ultimately shed contributing another pool of LPS to fecal excretion. Intraperitoneal LPS causes shedding of small intestinal epithelial cells in a Tnf receptor- (Tnfr-) dependent manner within 1.5 hours at doses as low as 0.125 mg/kg [27]. The rapid manifestation of epithelial shedding, preceded by the crypt appearance of LPS, suggests transmigration of intraperitoneal LPS across the visceral peritoneum and not only derived from circulation. The amelioration of splenic injury from the introduction of normal mesenteric lymph into LPS-treated mice indicates a role for mesenteric fluids in systemic inflammation [33]. Intestinal clearance of LPS causes intestinal permeability, oxidative stress, and intestinal mitochondrial damage and increases lipid peroxidation [34].

As shown in Figure 1, LPS initiates inflammation through toll-like receptor (TLR4) signaling that activates NFκB-mediated cytokine production including Tnfα, IL-6 and IL-1β [35]. Keap1 is a redox-sensing cytosolic inhibitor protein for the transcription factor Nrf2 that upregulates the expression a battery of antioxidant, anti-inflammatory, and DNA repair genes including heme oxygenase-1 (Ho-1) [36, 37]. In response to increasing intracellular oxidation status or the binding of other electrophiles, the conformation of Keap1 is altered, releasing Nrf2 to translocate to the nucleus, binding the antioxidant response element (ARE) in the promoter regions of target genes (Figure 2) [38]. Priming the Keap1-Nrf2-ARE pathway with dietary electrophilic phytochemicals increases the threshold to the initiation of inflammation and delays the activation of proinflammatory transcription factor NFκB [39–41]. The inhibitory role of Nrf2 has also been demonstrated in macrophages where it can bind ARE-independent DNA sequences in the promoter region of IL-6 and IL-1β, suppressing their transcription [42]. Additionally, LPS can physically disrupt red blood cell membranes releasing free heme with prooxidant potential [43]. In its enzyme role, inducible heme oxygenase-1 (Ho-1) degrades free heme to equimolar amounts of carbon monoxide (CO), free iron, and biliverdin. Biliverdin is enzymatically converted to bilirubin which forms an antioxidant redox couple, while CO is independently anti-inflammatory [44]. Upregulating Ho-1 is protective against intestinal inflammation and loss of barrier integrity [45–47] and maintains alternatively activated/M2 macrophage polarization [48–50], shifting the polarization of intestinal T cells towards a regulatory phenotype [51–53].

(a) Signaling

(b) Physicochemical

Figure 1

Effects of LPS. (1) LPS binding to the toll-like receptor-4 (TLR4) receptor initiates signaling to disrupt the inhibitor protein IKK association with proinflammation transcription factor NFκB. (2) Free NFκB translocates to the nucleus to increase the transcription of proinflammatory cytokines Tnfα, IL-6, IL-1β, etc. (3) LPS causes plasma membrane disruption in red blood cells releasing free heme. (4) Ho-1 breaks down free heme to equimolar amounts of CO, Fe, and biliverdin which is enzymatically converted to bilirubin, forming a redox couple.

Polyacetylenes are bioactive bisacetylenic phytooxylipins abundant not only in medicinal plants such as Notopterygium incisum (Qiang Huo) [54], Angelica sinensis (Dong Quai) [55, 56], and ginseng [57] but also in agricultural crops from the Apiaceae family [58], the most widely consumed of which is carrot [59, 60]. Falcarinol (FA) and falcarindiol (FD) are the most abundant carrot-derived polyacetylenes and have a demonstrated anti-inflammatory effect [60–62], in part by the suppression of NFκB [63]. FD has been shown to activate Nrf2 by S-alkylation of its inhibitor protein Keap1 [64]. FD pretreatment upregulated the antioxidant enzymes NADPH:quinone oxidoreductase (Nqo1) and glutathione-S-transferase (GST), protecting against a later oxidative challenge in both normal liver cells [65] and an in vivo mouse model examining the activity of these enzymes in the liver, small intestine, kidney, and lung, in part by reducing lipid peroxidation [66]. Ginseng-derived panaxynol, structurally identical to carrot-derived falcarinol, is an anti-inflammatory compound and potent activator of cardiac Nrf2 [57]. In humans, panaxynol reduces oxidative stress-induced plasma lipid peroxidation [67]. We set out to evaluate for the first time the protective effect of diet-achievable levels of FA against intestinal inflammation in comparison to sulforaphane (SF)—widely recognized as the most potent natural compound activator of the Nrf2/ARE pathway.

2. Methods

2.1. Animal Treatment

Three-month-old male CB57BL/6 mice (Charles River, St. Constant, QC, Canada) were individually housed in a temperature-controlled room on a reverse (12 : 12) light-dark cycle, fed a standard chow diet (Harlan Teklad, Mississauga, ON, Canada), with access to water ad libitum. Phytochemicals were prepared in 100% ethanol immediately before individual doses were prepared in peanut butter and allowed to evaporate overnight, refrigerated in a light-proof container. Twice per day for 7 days, 4 groups of mice received peanut butter (166 mg ± 0.01) with 5 mg/kg FA (CAS# 21852-80-2, Quality Phytochemicals LLC, East Brunswick, NJ, USA) (FA group), 5 mg/kg SF (CAS# 142825-10-3, Cayman Chemical, Ann Arbour, MI, USA) (SF group), or ethanol vehicle for the two control groups: a negative control (NC group) that was saline-treated and a positive control (PC group) that was lipopolysaccharide- (LPS-) treated. The chemical structures of FA and SF are shown in Figure 3. To elicit an immune response, the FA, SF, and PC groups of fasted animals ( per group) received an intraperitoneal injection of 5 mg/kg LPS on the eighth day and were sacrificed after 4 hours—a time point chosen for maximal intestinal inflammatory response [68, 69]. Plasma was collected by cardiac puncture, and tissues were removed and snap frozen in liquid nitrogen. All of the procedures conducted were approved by the University of Guelph Animal Care Committee and were in accordance with the guidelines of the Canadian Council on Animal Care.

2.2. Histological Analysis

Upper duodenal sections were flushed with saline and fixed in phosphate-buffered 10% formalin solution for 24 hours. Paraffin blocks were embedded, and 5 μm sections in longitudinal orientation were slide-mounted, and haematoxylin and eosin (H&E) staining was performed by the Animal Health Laboratory at the University of Guelph. Histomorphological evaluation of H&E-stained slides was scored by a professional veterinary pathologist (Animal Health Laboratory-Kempville) in a blinded fashion using the methods outlined by Erben et al. [70]. Slides were evaluated for the inflammatory cell infiltrate score (as per Table 8, Erben et al.), and a number of mitotic cells were counted in 10 contiguous 400x fields [70].

2.3. Plasma Cytokines

Plasma cytokines were measured using a magnetic bead-based sandwich immunoassay according to the manufacturer’s instructions (Bio-Plex Pro™ Mouse Cytokine 23-plex Assay, Bio-Rad Laboratories, Mississauga, Ontario). Antibody-coupled beads were incubated with plasma samples (1 : 3 dilution) in duplicate and incubated with biotinylated detection antibody to create a sandwich complex. Samples were subsequently incubated with streptavidin-phycoerythrin conjugate to serve as a fluorescent reporter. Beads were washed, and bound molecules were detected using a Bio-Plex 200 System (Bio-Rad Laboratories, Mississauga, Ontario).

2.4. PCR

mRNA was extracted from tissues using TRIzol according to the manufacturer’s instructions (Thermo Fisher Scientific). mRNA concentration was evaluated by measuring absorbance using a Nanodrop spectrophotometer (Nanodrop 2000, Thermo Fisher Scientific). For each sample, 1 μg of mRNA was incubated with DNase to remove genomic DNA and used for subsequent cDNA synthesis according to the manufacturer’s instructions (iScript gDNA Clear cDNA synthesis kit, Bio-Rad Laboratories, Mississauga, Ontario). Resulting cDNA was amplified by real-time RT-PCR (CFX Connect, Bio-Rad Laboratories, Mississauga, Ontario) with select primers using PCR reagents according to the manufacturer’s instructions (SsoAdvanced Universal SYBR Green Supermix, Bio-Rad Laboratories, Mississauga, Ontario). For each tissue, the geometric mean of 3 reference genes (Rps29, 18s, and Tbp) was used to calculate the delta Ct for each gene of interest.

2.5. Immunoblotting

Tissue samples were homogenized in cell lysis buffer (liver) or RIPA buffer (intestine) and centrifuged at 15,000 for 10 minutes at 4° C. Lysate supernatant was collected, and protein was quantified by bicinchoninic acid protein assay (Pierce Thermo Fisher Scientific) and measured with a plate reader (Molecular Devices, San Jose, USA). Protein concentration was standardized, and samples were separated in a 10% gel and transferred to PVDF membrane with a semidry electrophoretic transfer system (Bio-Rad Laboratories, Mississauga, Ontario). Membranes were incubated overnight with a 1 : 1000 dilution of primary antibody (Ho-1 and Nqo1, Abcam, Toronto, Canada), followed by a 1 : 3000 dilution of horseradish peroxidase-link secondary anti-mouse antibody (Cell Signaling Technology, Whitby, Canada). Blots were visualized with electrochemiluminescence reagent (Clarity Max, Bio-Rad Laboratories, Mississauga, Ontario), and images were captured with either FluorChem HD2 System (Cell Biosciences, San Jose, USA) or Gel Logic 6000 Pro (Carestream, Rochester, USA). Membranes were quantified using Image Studio™ Lite software (LI-COR Biosciences, Lincoln, USA) and normalized to either β-tubulin (liver) or total protein (intestine).

2.6. Lipid Peroxidation

Tissues were homogenized with 10 volumes of RIPA buffer containing protease and phosphatase inhibitors (Sigma-Aldrich P2714 and P5726, respectively) and centrifuged at 1600 for 10 minutes at 4°C. The supernatant was used undiluted in the TBARS assay (Cayman Chemical, Ann Arbor, USA) according to the manufacturer’s instructions. Briefly, the sample supernatant was combined with thiobarbituric acid assay reagents and boiled for 1 hour. Cooled sample preparations were loaded onto a 96-well plate and the absorbance read at 535 nm in a microplate reader (Molecular Devices, San Jose, USA), and lipid peroxides were interpolated from a malondialdehyde standard curve.

2.7. Statistical Analysis

Data were analyzed by one-way analysis of variance (ANOVA) followed by Tukey’s posttest method to compare group means (“” for ANOVA-derived values and “” for those derived from the posttest). All results with were accepted as statistically significant; marginally significant results (; i.e., ) are also mentioned. Qualitative scoring for intestinal inflammation was analyzed by Kruskal-Wallis one way analysis of variance, and Dunn’s test was used to evaluate the pairwise mean rank difference. All data were analyzed with GraphPad Prism software (version 7).

3. Results

3.1. Falcarinol Was a Potent Reducer of Intestinal Inflammation

Intestinal proinflammatory gene expression peaks between 4 and 6 hours after LPS injection [71], and maximal circulating proinflammatory cytokines Tnfα, IL-6, and IL-1 occur closer to 4 hours of postinjection [68, 72], so we chose the time point of 4 hours to best capture the acute intestinal and systemic inflammatory response. As shown in Figure 4(a), in the jejunum, both phytochemicals falcarinol (FA) and sulforaphane (SF) reduced the expression of LPS-induced proinflammatory genes, but FA was consistently more effective than SF. IL-6 showed the greatest magnitude of change among the inflammatory genes, increasing 103.6-fold for LPS treatment alone (positive control (PC)) and 85.2-fold for SF ( for both), whereas for FA, the increase was prevented and the expression was not significantly different from the LPS-untreated negative control (NC). This pattern repeated for Tnfα, its receptor (Tnfr), and Ifnγ. Tnfα expression increased by 48.8-fold for PC () and 24.6-fold for SF (), and Tnfr was increased by 5.1-fold in PC () and 2.6-fold in SF (), but for FA-treated mice, the increases were prevented and not significantly different from the negative control group. Ifnγ mRNA increased by 22.3-fold in PC (), but there was no significant increase for either phytochemical-treated groups. Stat3 increased in all LPS-treated groups, increasing by 3.6-fold in PC, 2.8-fold in SF (both ), and 2-fold in FA (). Stat3 was significantly lower for FA than both PC and SF ( and , respectively). As shown in Figure 5, IL-10 and its receptor (IL-10R) were also significantly increased by LPS treatment and the LPS response was reduced by both phytochemical treatments. IL-10 expression was increased by 17.7-, 13.1-, and 9.5-fold in PC, SF, and FA, respectively (), whereas its receptor increased only for PC (by 1.6-fold) and decreased with phytochemical treatment (both to 0.7-fold, ). Altogether, the phytochemical pretreatment effectively reduced the magnitude of intestinal proinflammatory gene expression with FA showing more potency than SF.

(a)

(b)

(a)

(b)

3.2. Phytochemicals Had a Minor Effect on Hepatic Inflammation

At 4 hours of post LPS injection, the effect on hepatic inflammatory gene expression was more subdued than in the intestine. As shown in Figure 4(b), the main inflammatory genes (IL-6, Tnfα, and Ifnγ) were all increased by LPS treatment and the phytochemical pretreatments showed no reductions in their expression. In fact, IL-6 had the greatest magnitude of increase for all LPS groups with the highest increase for SF (). Tnfr mRNA was upregulated by 2.4-fold and 2.5-fold for SF and PC, respectively (both ), that was presented in the FA group. Stat3 was significantly upregulated in all LPS-treated groups (). SF and PC both increased by 4.8-fold (both ). Differently from SF, FA caused the most conservative increase in Stat3 (3.8-fold, ), showing some reducing effects.

3.3. Downregulated Expression of Intestinal Nrf2 Pathway Genes Was Not Rescued with Pretreatments

We also evaluated the effect of phytochemicals on the expression of Nrf2, Keap1, and their responsive genes Hmox1 and Nqo1 in both the intestine and the liver (Figure 6). In the intestine, the expression of Nrf2 was 3-fold downregulated by LPS () and not rescued by phytochemical pretreatment at 4 hours of postinjection. Keap1 was significantly upregulated only in PC by 1.6-fold (). We anticipated an increased expression of Nrf2 target genes by both phytochemical pretreatments but observed that only heme oxygenase-1 (Hmox1) was significantly increased only for FA by 8.9-fold above control (). Nqo1 (Figure 6) and Muc-2 (not shown) gene expression also were not significantly changed by LPS with or without phytochemical pretreatments.

(a)

(b)

3.4. Falcarinol but Not Sulforaphane Stimulated Expression of Hepatic Nrf2 Pathway

In contrast, in the liver, LPS had no impact on the Nrf2 pathway (Figure 6(b)). In fact, the FA pretreatment resulted in a significant increase of Nrf2 mRNA (), and Keap1 was significantly upregulated only in the SF and PC groups (2.0- and 2.1-fold, respectively; both ). Similarly, Hmox1 was significantly increased only in the FA-treated group (by 6.5-fold, ), and there was no difference in expression between the SF and PC groups. Nqo1 expression was not significantly affected by either LPS or phytochemicals in the liver.

3.5. Falcarinol but Not Sulforaphane Increased Intestinal and Liver Heme Oxygenase-1 Protein

Interestingly, Ho-1 and Nqo1 proteins followed a similar expression pattern with respect to mRNA in both the intestine and the liver (Figure 7). The intestinal Ho-1 protein was significantly increased with FA (1.83-fold, ), while there was no effect of SF or PC on Ho-1 protein. Similarly, the largest increase in hepatic Ho-1 protein was obtained only with FA (16.4-fold; ). On the other hand, the intestinal Nqo1 protein was increased with all treatments but was significant only in the LPS PC group (2.18-fold, ). There was no effect of either phytochemical or LPS treatment on the liver Nqo1 protein.

(a)

(b)

3.6. Falcarinol Pretreatment Specifically Reduced Initial-Phase Plasma Cytokines

Eosinophils are the first immune cells to be recruited to the site of injury in response to locally produced eotaxin, and are followed by more numerous neutrophils and macrophages [73]. As shown in Figure 8, eotaxin increased 5.4-fold for LPS alone (, PC) and it was attenuated with FA, which only showed a 4.1-fold increase (), but not with SF (5.0-fold, ) demonstrating that FA was able to show some protective effects in the initial phases of the LPS response. Granulocyte-macrophage colony-stimulating factor (GM-CSF) acts to recruit eosinophils and macrophages but is inhibitory to neutrophils [74]; GM-CSF was significantly increased only for SF and PC, by 5.6-fold and 6.7-fold, respectively (). IL-12p40 was significantly upregulated only for SF (by 90.2-fold, ).

(a)

(b)

(c)

(d)

The plasma inflammatory cytokines (IL-1α, IL-1β, IL-6, and Ifnγ) were all significantly upregulated by LPS treatment, but there was no effect of phytochemical pretreatment on the magnitude of the response seen at the 4-hour time point. Tnfα was significantly increased only in the FA group (by 8.4-fold, ). Other inflammatory factors IL-13, MIP-1α, and MIP-1β were significantly increased but without a protective effect of phytochemical treatment; similarly, the regulatory cytokines IL-3, IL-4, and IL-10 were all significantly upregulated by LPS with no effect of phytochemical pretreatment. All cytokines were increased in the plasma after LPS injection, with the exception of IL-9 which was not detectable in all samples. Changes were not significant for IL-2, IL-5, IL-17, KC, MCP-1, RANTES, or IL-12p70.

3.7. Falcarinol Specifically Reduced Lipid Peroxidation in the Mesentery

As shown in Figure 8, LPS had no significant effect on lipid peroxidation in the plasma, jejunum, or mesentery at 4 hours of postinjection; however, TBARS was significantly lower in the mesentery of the FA-treated mice ().

3.8. Falcarinol Completely Attenuated Inflammatory Cell Infiltration and Reduced Epithelial Turnover in the Intestine

Qualitative scores for inflammatory cell infiltrate and epithelial damage were moderate 4 h after LPS treatment, ranging from 0 to 3 on a scale of 8. FA however completely attenuated LPS-induced inflammatory cell infiltration in the duodenum (Figure 9). Remarkably, despite LPS treatment, the score for FA was lower even than saline-treated NC. Both SF and PC scored similarly to NC; differences were only significant between FA and SF (mean ranks: 2.5 and 9.0, respectively, ). The number of mitotic cells in the intestinal epithelium is a marker for the epithelial cell turnover rate [32, 75]. Results only approached significance between NC and PC (). The mean numbers of mitotic cells counted in 10 contiguous 400x fields were 24, 33, 45, and 63 for NC, FA, SF, and PC, respectively (Figure 9). This study did not observe shedding directly, but histology revealed the architecture of PC duodenum to be so poor due to shortened villi (crypt : villus ratio is ~1 : 3 for PC as compared to 7–12 for the other groups) in which further morphological study was not possible. This effect was not seen in the LPS-treated groups that received phytochemical pretreatment.

4. Discussion

The anticancer effects of FA are its best characterized bioactive property [76–83]. FA also has positive metabolic effects. In vitro, FA improves insulin signaling in insulin-resistant porcine myotubes [84] and increases glucose uptake in normal porcine myotubes and adipocytes, as well as inhibiting adipocyte differentiation [85]. Interestingly, falcarindiol does not inhibit adipocyte differentiation but is a more potent PPARγ agonist than FA which requires a higher dose to initiate an effect [54, 85]. FA stimulates normal intestinal cell growth at physiological doses, whereas carotenoids have no effect [86], and carrot juice has an anti-inflammatory effect in vitro intestinal cells [87]. FA also has anticomplement activity [88] and modulates GABA_A receptor activation [89].

In this study, we observed that the local effect of LPS on the intestine produced a greater response of inflammatory gene expression than in the liver, which would be expected to experience a lower dose of LPS derived from systemic circulation as opposed to directly from the intraperitoneal space. Additionally, the protective effect of the phytochemicals and falcarinol, in particular, was more pronounced in the intestine than in the liver. Intestinal cells would have been exposed to the full phytochemical dose over a short amount of time—a higher effective dose that would be available to cells relying on systemic circulation for phytochemical exposure such as the liver. The novel finding in this study is that falcarinol was more effective than sulforaphane in attenuating inflammatory gene expression in the intestine and to a lesser degree in the liver.

We also examined the effect of phytochemicals on Nrf2-activated targets, Ho-1 and Nqo1. Heme oxygenase-1 (Ho-1, Hmox1) has an emerging role in attenuating intestinal inflammation and protecting intestinal barrier integrity by upregulating the expression of tight junction proteins [47] and attenuating inflammation-induced intestinal permeability [46]. Prior Ho-1 upregulation protected intestinal barrier integrity by upregulating tight junction proteins, reducing apoptosis, activating Nrf2, and reducing NFκB activation resulting from abdominal surgery in a rat model [90] and associated oxidative stress [91, 92]. FA, but not SF, significantly upregulated Hmox1 in both the liver and intestine, whereas Nqo1 expression was not affected by phytochemical. A unique characteristic of the Nqo1 promoter is the number of ARE sequences. Rather than rendering Nqo1 more Nrf2-sensitive due to the increased number of ARE contributing to its regulation, it appears that it is more likely that Nqo1 requires more intense Nrf2 exposure to affect transcriptional activation than Hmox1. We demonstrated that Hmox1 is more sensitive to Nrf2 activation than Nqo1 in the liver and intestine which was also reflected in protein levels. Nqo1 protein levels were only significantly elevated in the intestine of PC, whereas in the liver, neither LPS nor phytochemical pretreatment showed an effect. Ho-1 protein levels were significantly increased from NC in both the liver and the intestine only in FA-treated mice, with no difference between the SF and the PC groups. Notably, this effect was only seen with FA-treated mice and not those treated with SF. This unique effect of FA is another novel finding in this study.

FA attenuated circulating eotaxin and GM-CSF (a proinflammatory inducer of M1 phenotype [93]) as compared to other LPS-treated groups, which could potentially translate to reduced immune cell recruitment, but cell trafficking was not evaluated in this study. Lipid peroxidation was not increased at 4 hours after LPS injection in any of the plasma, intestine, or mesentery; however, FA pretreatment reduced basal lipid peroxidation in the mesentery, which may be a contributing factor to the surprising reduction of inflammatory cell infiltration in FA duodena.

Glutathione-S-transferase is a phase II detoxification enzyme that conjugates electrophiles [94]. Sulforaphane is absorbed into intestinal cells as a glutathione conjugate [95], an interaction that is promoted by intracellular glutathione transferases [96] or a direct interaction with lumenal glutathione derived from the diet [97] or bile [98]. It is known that a portion of absorbed sulforaphane is secreted back into the intestine as a glutathione conjugate, reducing its bioavailability to 74% by some estimates [99]. The bioavailability of polyacetylenes has been demonstrated [100, 101], and they have been shown to bind human serum albumin for circulatory distribution [102], but we are not aware of any studies specific to their uptake mechanisms. Due to the electrophilicity of polyacetylenes; these mechanisms may be similar to SF, and possibly differential uptake efficiencies may contribute to the greater effectiveness of FA in vivo.

Normal epithelial cell loss from the villi tips is replaced by cells newly differentiated from crypt stem cells; a balance between cell loss and regeneration maintains intestinal barrier integrity. Accelerated mitosis in the epithelial layer is suggestive of shedding since there would be an increased need for regeneration to replace lost cells at the villus tip. LPS-treated groups had more mitotic cells than NC (1.38- and 1.88-fold more for FA and SF, respectively); PC had the most mitotic cells (2.63-fold more than NC) but did not reach significance (), demonstrating the superior effect of FA over SF in protecting intestinal integrity. While LPS treatment did not substantively increase the qualitative score of inflammatory cell infiltration (mild to moderate infiltration in NC, SF, and PC), remarkably, FA did not show any infiltration despite LPS treatment (score = 0).

While it is possible that FA is a more potent activator of Nrf2 than sulforaphane, there may be other effects of FA that are responsible. Endocannabinoid signaling is involved in maintaining intestinal barrier integrity. Antagonism of cannabinoid type 1 receptor (CB₁R) reduced intestinal inflammation and permeability in a diet-induced obesity model, attenuating metabolic endotoxemia and adipose inflammation and improving insulin resistance [103]. Pretreatment of the apical but not basolateral side of a Caco-2 cell monolayer prevented the cytokine-induced increase in intestinal permeability mediated by the antagonism of CB₁R [104]. Dietary (apical side exposure) FA is likely protective of the intestinal epithelium since it is a covalent CB₁R antagonist [105]; we are unaware of any studies directly evaluating sulforaphane for potential CB₁R antagonism.

The current study evaluated the anti-inflammatory and antioxidant effects of isolated bioactive compounds available in the diet and their role in the prevention of inflammation (commonly understood to play an important role in the development of most chronic diseases) and more specifically in the context of intestinal inflammation and the maintenance of intestinal barrier integrity. Intestinal inflammation is particularly relevant since it provides the milieu for the polarization of naive T cells and other immune cells which have wider implications for the overall immune tone. The degradation of the intestinal barrier is gaining recognition as another early deviation from homeostasis contributing to the development of more serious and widely divergent diseases including some autoimmune conditions, food allergies, obesity, endotoxemia, chronic inflammation, and even intense exercise. Furthermore, our use of low/diet-achievable doses (5 mg/kg) as opposed to the commonly used default for studies of this type (100 mg/kg), which is a pharmaceutical or supplemental dose, make our findings all the more relevant since these effects are seen at dietary levels of exposure.

In conclusion, we have demonstrated the superior effectiveness of FA over SF at attenuating LPS-induced intestinal gene expression and to a lesser degree in the liver. FA was uniquely effective at upregulating Nrf2-target Ho-1 in both the intestine and the liver and attenuating some initial phase proinflammatory cytokines. FA also reduced inflammatory cell infiltration in the duodenum below even negative control and reduced basal mesenteric lipid peroxidation. These results suggest that the efficacy of FA may be fruitful to explore for prevention and treatment in inflammatory pathologies of the GI tract and in supporting the maintenance of intestinal barrier integrity due to the superiority of FA at upregulating Ho-1 to the anti-inflammatory and antioxidant effect demonstrated in the current study.

Data Availability

The data used to support the findings of this study are available from the corresponding author upon request.

Conflicts of Interest

The authors declare that there is no conflict of interest regarding the publication of this paper.

Acknowledgments

This research is funded by the Agri-Innovation Program of Agriculture and Agri-Food Canada’s Growing Forward 2 Policy Framework (a federal-provincial-territorial initiative), Loblaw Companies Ltd., and the Carrot Common through the Organic Science Cluster II, an industry-supported research and development endeavour initiated by the Organic Agriculture Centre of Canada at Dalhousie University in collaboration with the Organic Federation of Canada.

References

J. R. Turner, “Intestinal mucosal barrier function in health and disease,” Nature Reviews. Immunology, vol. 9, no. 11, pp. 799–809, 2009.
View at: Publisher Site | Google Scholar
L. S. Kaminsky and Q.-Y. Zhang, “The small intestine as a xenobiotic-metabolizing organ,” Drug Metabolism and Disposition, vol. 31, no. 12, pp. 1520–1525, 2003.
View at: Publisher Site | Google Scholar
P. Brandtzaeg, “The gut as communicator between environment and host: immunological consequences,” European Journal of Pharmacology, vol. 668, pp. S16–S32, 2011.
View at: Publisher Site | Google Scholar
C. Lopez-Garcia, A. M. Klein, B. D. Simons, and D. J. Winton, “Intestinal stem cell replacement follows a pattern of neutral drift,” Science, vol. 330, no. 6005, pp. 822–825, 2010.
View at: Publisher Site | Google Scholar
J. Visser, J. Rozing, A. Sapone, K. Lammers, and A. Fasano, “Tight junctions, intestinal permeability, and autoimmunity,” Annals of the New York Academy of Sciences, vol. 1165, no. 1, pp. 195–205, 2009.
View at: Publisher Site | Google Scholar
R. Kiesslich, C. A. Duckworth, D. Moussata et al., “Local barrier dysfunction identified by confocal laser endomicroscopy predicts relapse in inflammatory bowel disease,” Gut, vol. 61, no. 8, pp. 1146–1153, 2012.
View at: Publisher Site | Google Scholar
J.-F. Turcotte, K. Wong, S. J. Mah et al., “Increased epithelial gaps in the small intestine are predictive of hospitalization and surgery in patients with inflammatory bowel disease,” Clinical and Translational Gastroenterology, vol. 3, no. 7, pp. e19–e16, 2012.
View at: Publisher Site | Google Scholar
Q. Mu, J. Kirby, C. M. Reilly, and X. M. Luo, “Leaky gut as a danger signal for autoimmune diseases,” Frontiers in Immunology, vol. 8, p. 598, 2017.
View at: Publisher Site | Google Scholar
C. Bleau, A. D. Karelis, D. H. St-Pierre, and L. Lamontagne, “Crosstalk between intestinal microbiota, adipose tissue and skeletal muscle as an early event in systemic low-grade inflammation and the development of obesity and diabetes,” Diabetes/Metabolism Research and Reviews, vol. 31, no. 6, pp. 545–561, 2015.
View at: Publisher Site | Google Scholar
E. A. Deitch, “Intestinal permeability is increased in burn patients shortly after injury,” British Journal of Surgery, vol. 77, no. 5, pp. 587–592, 1990.
View at: Publisher Site | Google Scholar
D. S. Walsh, P. Thavichaigarn, C. Dheeradhada et al., “Prolonged alteration in gut permeability following nonthermal injury,” Injury, vol. 27, no. 7, pp. 491–494, 1996.
View at: Publisher Site | Google Scholar
Z. M. Earley, S. Akhtar, S. J. Green et al., “Burn injury alters the intestinal microbiome and increases gut permeability and bacterial translocation,” PLoS One, vol. 10, no. 7, pp. e0129996–e0129916, 2015.
View at: Publisher Site | Google Scholar
J. S. Aranow and M. P. Fink, “Determinants of intestinal barrier failure in critical illness,” British Journal of Anaesthesia, vol. 77, no. 1, pp. 71–81, 1996.
View at: Publisher Site | Google Scholar
X. Gao, J. Zhang, D. Yang, Q. Tao, L. Liu, and J. Guo, “Effects of heme oxygenase-1 in the intestine on the intestinal barrier function of rats with hemorrhagic shock,” International Journal of Clinical and Experimental Medicine, vol. 9, no. 9, pp. 17367–17376, 2016.
View at: Google Scholar
M. Lamprecht, S. Bogner, K. Steinbauer et al., “Effects of zeolite supplementation on parameters of intestinal barrier integrity, inflammation, redoxbiology and performance in aerobically trained subjects,” Journal of the International Society of Sports Nutrition, vol. 12, no. 1, p. 40, 2015.
View at: Publisher Site | Google Scholar
N. Vargas and F. Marino, “Heat stress, gastrointestinal permeability and interleukin-6 signaling — implications for exercise performance and fatigue,” Temperature, vol. 3, no. 2, pp. 240–251, 2016.
View at: Publisher Site | Google Scholar
K. Dokladny, M. N. Zuhl, and P. L. Moseley, “Intestinal epithelial barrier function and tight junction proteins with heat and exercise,” Journal of Applied Physiology, vol. 120, no. 6, pp. 692–701, 2016.
View at: Publisher Site | Google Scholar
L. M. JanssenDuijghuijsen, M. Mensink, K. Lenaerts et al., “The effect of endurance exercise on intestinal integrity in well-trained healthy men,” Physiological Reports, vol. 4, no. 20, article e12994, 2016.
View at: Publisher Site | Google Scholar
D. S. March, T. Marchbank, R. J. Playford, A. W. Jones, R. Thatcher, and G. Davison, “Intestinal fatty acid-binding protein and gut permeability responses to exercise,” European Journal of Applied Physiology, vol. 117, no. 5, pp. 931–941, 2017.
View at: Publisher Site | Google Scholar
J. C. Mathison and R. J. Ulevitch, “The clearance, tissue distribution, and cellular localization of intravenously injected lipopolysaccharide in rabbits,” The Journal of Immunology, vol. 123, no. 5, pp. 2133–2143, 1979.
View at: Google Scholar
Z. Yao, J. M. Mates, A. M. Cheplowitz et al., “Blood-borne lipopolysaccharide is rapidly eliminated by liver sinusoidal endothelial cells via high-density lipoprotein,” The Journal of Immunology, vol. 197, no. 6, pp. 2390–2399, 2016.
View at: Publisher Site | Google Scholar
M. A. Freudenberg, N. Freudenberg, and C. Galanos, “Time course of cellular distribution of endotoxin in liver, lungs and kidneys of rats,” British Journal of Experimental Pathology, vol. 63, no. 1, pp. 56–65, 1982.
View at: Google Scholar
B. Shao, M. Lu, S. C. Katz et al., “A host lipase detoxifies bacterial lipopolysaccharides in the liver and spleen,” The Journal of Biological Chemistry, vol. 282, no. 18, pp. 13726–13735, 2007.
View at: Publisher Site | Google Scholar
Y. Mimura, S. Sakisaka, M. Harada, M. Sata, and K. Tanikawa, “Role of hepatocytes in direct clearance of lipopolysaccharide in rats,” Gastroenterology, vol. 109, no. 6, pp. 1969–1976, 1995.
View at: Publisher Site | Google Scholar
E. d’Hennezel, S. Abubucker, L. O. Murphy, and T. W. Cullen, “Total lipopolysaccharide from the human gut microbiome silences toll-like receptor signaling,” mSystems, vol. 2, no. 6, article e00046-17, 2017.
View at: Publisher Site | Google Scholar
A. Gnauck, R. G. Lentle, and M. C. Kruger, “The characteristics and function of bacterial lipopolysaccharides and their endotoxic potential in humans,” International Reviews of Immunology, vol. 35, no. 3, pp. 189–218, 2016.
View at: Publisher Site | Google Scholar
J. M. Williams, C. A. Duckworth, A. J. M. Watson et al., “A mouse model of pathological small intestinal epithelial cell apoptosis and shedding induced by systemic administration of lipopolysaccharide,” Disease Models & Mechanisms, vol. 6, no. 6, pp. 1388–1399, 2013.
View at: Publisher Site | Google Scholar
H. Inagawa, C. Kohchi, and G. Soma, “Oral administration of lipopolysaccharides for the prevention of various diseases: benefit and usefulness,” Anticancer Research, vol. 31, no. 7, pp. 2431–2436, 2011.
View at: Google Scholar
B. Kleine, M. A. Freudenberg, and C. Galanos, “Excretion of radioactivity in faeces and urine of rats injected with 3H,14C-lipopolysaccharide,” British Journal of Experimental Pathology, vol. 66, no. 3, pp. 303–308, 1985.
View at: Google Scholar
M. A. Freudenberg, B. Kleine, and C. Galanos, “The fate of lipopolysaccharide in rats: evidence for chemical alteration in the molecule,” Reviews of Infectious Diseases, vol. 6, no. 4, pp. 483–487, 1984.
View at: Publisher Site | Google Scholar
Y. Ge, R. M. Ezzell, and H. S. Warren, “Localization of endotoxin in the rat intestinal epithelium,” The Journal of Infectious Diseases, vol. 182, no. 3, pp. 873–881, 2000.
View at: Publisher Site | Google Scholar
C.-W. Lai, T.-L. Sun, W. Lo et al., “Shedding-induced gap formation contributes to gut barrier dysfunction in endotoxemia,” Journal of Trauma and Acute Care Surgery, vol. 74, no. 1, pp. 203–213, 2013.
View at: Publisher Site | Google Scholar
L.-M. Zhang, W. Song, H. Cui et al., “Normal mesenteric lymph ameliorates lipopolysaccharide challenge-induced spleen injury,” Acta Cirúrgica Brasileira, vol. 30, no. 9, pp. 604–610, 2015.
View at: Publisher Site | Google Scholar
S. Cao, Q. Zhang, C. C. Wang et al., “LPS challenge increased intestinal permeability, disrupted mitochondrial function and triggered mitophagy of piglets,” Innate Immunity, vol. 24, no. 4, pp. 221–230, 2018.
View at: Publisher Site | Google Scholar
Y.-C. Lu, W.-C. Yeh, and P. S. Ohashi, “LPS/TLR4 signal transduction pathway,” Cytokine, vol. 42, no. 2, pp. 145–151, 2008.
View at: Publisher Site | Google Scholar
A. Kobayashi, M. I. Kang, H. Okawa et al., “Oxidative stress sensor Keap1 functions as an adaptor for Cul3-based E3 ligase to regulate proteasomal degradation of Nrf2,” Molecular and Cellular Biology, vol. 24, no. 16, pp. 7130–7139, 2004.
View at: Publisher Site | Google Scholar
A. T. Dinkova-Kostova, R. V. Kostov, and P. Canning, “Keap1, the cysteine-based mammalian intracellular sensor for electrophiles and oxidants,” Archives of Biochemistry and Biophysics, vol. 617, pp. 84–93, 2017.
View at: Publisher Site | Google Scholar
Y. Watai, A. Kobayashi, H. Nagase et al., “Subcellular localization and cytoplasmic complex status of endogenous Keap1,” Genes to Cells, vol. 12, no. 10, pp. 1163–1178, 2007.
View at: Publisher Site | Google Scholar
Y.-J. Surh, J. Kundu, and H.-K. Na, “Nrf2 as a master redox switch in turning on the cellular signaling involved in the induction of cytoprotective genes by some chemopreventive phytochemicals,” Planta Medica, vol. 74, no. 13, pp. 1526–1539, 2008.
View at: Publisher Site | Google Scholar
W. Li, T. O. Khor, C. Xu et al., “Activation of Nrf2-antioxidant signaling attenuates NFκB-inflammatory response and elicits apoptosis,” Biochemical Pharmacology, vol. 76, no. 11, pp. 1485–1489, 2008.
View at: Publisher Site | Google Scholar
A. Stefanson and M. Bakovic, “Dietary regulation of Keap1/Nrf2/ARE pathway: focus on plant-derived compounds and trace minerals,” Nutrients, vol. 6, no. 9, pp. 3777–3801, 2014.
View at: Publisher Site | Google Scholar
E. H. Kobayashi, T. Suzuki, R. Funayama et al., “Nrf2 suppresses macrophage inflammatory response by blocking proinflammatory cytokine transcription,” Nature Communications, vol. 7, article 11624, 2016.
View at: Publisher Site | Google Scholar
S. Brauckmann, K. Effenberger-Neidnicht, H. de Groot et al., “Lipopolysaccharide-induced hemolysis: evidence for direct membrane interactions,” Scientific Reports, vol. 6, no. 1, article 35508, 2016.
View at: Publisher Site | Google Scholar
S. Z. Sheikh, R. A. Hegazi, T. Kobayashi et al., “An anti-inflammatory role for carbon monoxide and heme oxygenase-1 in chronic Th2-mediated murine colitis,” The Journal of Immunology, vol. 186, no. 9, pp. 5506–5513, 2011.
View at: Publisher Site | Google Scholar
F. Tamion, V. Richard, S. Renet, and C. Thuillez, “Intestinal preconditioning prevents inflammatory response by modulating heme oxygenase-1 expression in endotoxic shock model,” American Journal of Physiology-Gastrointestinal and Liver Physiology, vol. 293, no. 6, pp. G1308–G1314, 2007.
View at: Publisher Site | Google Scholar
R. Akagi, M. Akagi, Y. Hatori, and S. Inouye, “Prevention of barrier disruption by heme oxygenase-1 in intestinal bleeding model,” Biological & Pharmaceutical Bulletin, vol. 39, no. 6, pp. 1007–1012, 2016.
View at: Publisher Site | Google Scholar
L. Zhang and Z. Zhang, “The protective effect of heme oxygenase-1 against intestinal barrier dysfunction in cholestatic liver injury is associated with NF-κB inhibition,” Molecular Medicine, vol. 23, no. 1, p. 1, 2017.
View at: Publisher Site | Google Scholar
C. Chauveau, S. Rémy, P. J. Royer et al., “Heme oxygenase-1 expression inhibits dendritic cell maturation and proinflammatory function but conserves IL-10 expression,” Blood, vol. 106, no. 5, pp. 1694–1702, 2005.
View at: Publisher Site | Google Scholar
E. Sierra-Filardi, M. A. Vega, P. Sánchez-Mateos, A. L. Corbí, and A. Puig-Kröger, “Heme oxygenase-1 expression in M-CSF-polarized M2 macrophages contributes to LPS-induced IL-10 release,” Immunobiology, vol. 215, no. 9-10, pp. 788–795, 2010.
View at: Publisher Site | Google Scholar
Y. Naito, T. Takagi, and Y. Higashimura, “Heme oxygenase-1 and anti-inflammatory M2 macrophages,” Archives of Biochemistry and Biophysics, vol. 564, pp. 83–88, 2014.
View at: Publisher Site | Google Scholar
S. S. Lee, W. Gao, S. Mazzola et al., “Heme oxygenase-1, carbon monoxide, and bilirubin induce tolerance in recipients toward islet allografts by modulating T regulatory cells,” The FASEB Journal, vol. 21, no. 13, pp. 3450–3457, 2007.
View at: Publisher Site | Google Scholar
S. Schulz, K. M. Chisholm, H. Zhao et al., “Heme oxygenase-1 confers protection and alters T-cell populations in a mouse model of neonatal intestinal inflammation,” Pediatric Research, vol. 77, no. 5, pp. 640–648, 2015.
View at: Publisher Site | Google Scholar
V. Vijayan, F. A. D. T. G. Wagener, and S. Immenschuh, “The macrophage heme-heme oxygenase-1 system and its role in inflammation,” Biochemical Pharmacology, vol. 153, pp. 159–167, 2018.
View at: Publisher Site | Google Scholar
A. G. Atanasov, M. Blunder, N. Fakhrudin et al., “Polyacetylenes from Notopterygium incisum–new selective partial agonists of peroxisome proliferator-activated receptor-gamma,” PLoS One, vol. 8, no. 4, pp. e61755–e61759, 2013.
View at: Publisher Site | Google Scholar
J. Liu, S. Zschocke, E. Reininger, and R. Bauer, “Inhibitory effects of Angelica pubescens f. biserrata on 5-lipoxygenase and cyclooxygenase,” Planta Medica, vol. 64, no. 06, pp. 525–529, 1998.
View at: Publisher Site | Google Scholar
T. Uto, N. H. Tung, R. Taniyama, T. Miyanowaki, O. Morinaga, and Y. Shoyama, “Anti-inflammatory activity of constituents isolated from aerial part of Angelica acutiloba Kitagawa,” Phytotherapy Research, vol. 29, no. 12, pp. 1956–1963, 2015.
View at: Publisher Site | Google Scholar
C. Qu, B. Li, Y. Lai et al., “Identifying panaxynol, a natural activator of nuclear factor erythroid-2 related factor 2 (Nrf2) from American ginseng as a suppressor of inflamed macrophage-induced cardiomyocyte hypertrophy,” Journal of Ethnopharmacology, vol. 168, pp. 326–336, 2015.
View at: Publisher Site | Google Scholar
C. Zidorn, K. Jöhrer, M. Ganzera et al., “Polyacetylenes from the Apiaceae vegetables carrot, celery, fennel, parsley, and parsnip and their cytotoxic activities,” Journal of Agricultural and Food Chemistry, vol. 53, no. 7, pp. 2518–2523, 2005.
View at: Publisher Site | Google Scholar
L. Schmiech, C. Alayrac, B. Witulski, and T. Hofmann, “Structure determination of bisacetylenic oxylipins in carrots (Daucus carotaL.) and enantioselective synthesis of falcarindiol,” Journal of Agricultural and Food Chemistry, vol. 57, no. 22, pp. 11030–11040, 2009.
View at: Publisher Site | Google Scholar
C. Dawid, F. Dunemann, W. Schwab, T. Nothnagel, and T. Hofmann, “Bioactive C₁₇-polyacetylenes in carrots (Daucus carota L.): current knowledge and future perspectives,” Journal of Agricultural and Food Chemistry, vol. 63, no. 42, pp. 9211–9222, 2015.
View at: Publisher Site | Google Scholar
B. T. Metzger, D. M. Barnes, and J. D. Reed, “Purple carrot (Daucus carota L.) polyacetylenes decrease lipopolysaccharide-induced expression of inflammatory proteins in macrophage and endothelial cells,” Journal of Agricultural and Food Chemistry, vol. 56, no. 10, pp. 3554–3560, 2008.
View at: Publisher Site | Google Scholar
H. Kang, T. S. Bang, J. W. Lee et al., “Protective effect of the methanol extract from Cryptotaenia japonica Hassk. against lipopolysaccharide-induced inflammation in vitro and in vivo,” BMC Complementary and Alternative Medicine, vol. 12, no. 1, p. 199, 2012.
View at: Publisher Site | Google Scholar
Y.-J. Shiao, Y. L. Lin, Y. H. Sun, C. W. Chi, C. F. Chen, and C. N. Wang, “Falcarindiol impairs the expression of inducible nitric oxide synthase by abrogating the activation of IKK and JAK in rat primary astrocytes,” British Journal of Pharmacology, vol. 144, no. 1, pp. 42–51, 2009.
View at: Publisher Site | Google Scholar
T. Ohnuma, S. Nakayama, E. Anan, T. Nishiyama, K. Ogura, and A. Hiratsuka, “Activation of the Nrf2/ARE pathway via S-alkylation of cysteine 151 in the chemopreventive agent-sensor Keap1 protein by falcarindiol, a conjugated diacetylene compound,” Toxicology and Applied Pharmacology, vol. 244, no. 1, pp. 27–36, 2010.
View at: Publisher Site | Google Scholar
T. Ohnuma, T. Komatsu, S. Nakayama, T. Nishiyama, K. Ogura, and A. Hiratsuka, “Induction of antioxidant and phase 2 drug-metabolizing enzymes by falcarindiol isolated from Notopterygium incisum extract, which activates the Nrf2/ARE pathway, leads to cytoprotection against oxidative and electrophilic stress,” Archives of Biochemistry and Biophysics, vol. 488, no. 1, pp. 34–41, 2009.
View at: Publisher Site | Google Scholar
T. Ohnuma, E. Anan, R. Hoashi et al., “Dietary diacetylene falcarindiol induces phase 2 drug-metabolizing enzymes and blocks carbon tetrachloride-induced hepatotoxicity in mice through suppression of lipid peroxidation,” Biological & Pharmaceutical Bulletin, vol. 34, no. 3, pp. 371–378, 2011.
View at: Publisher Site | Google Scholar
H. M. Al-Kuraishy and A. I. Al-Gareeb, “Eustress and malondialdehyde (MDA): role of Panax ginseng: randomized placebo controlled study,” Iranian Journal of Psychiatry, vol. 12, no. 3, pp. 194–200, 2017.
View at: Google Scholar
K. Tateda, T. Matsumoto, S. Miyazaki, and K. Yamaguchi, “Lipopolysaccharide-induced lethality and cytokine production in aged mice,” Infection and Immunity, vol. 64, no. 3, pp. 769–774, 1996.
View at: Google Scholar
H. Vedder, W. Schreiber, A. Yassouridis, S. Gudewill, C. Galanos, and T. Pollmächer, “Dose-dependence of bacterial lipopolysaccharide (LPS) effects on peak response and time course of the immune-endocrine host response in humans,” Inflammation Research, vol. 48, no. 2, pp. 67–74, 1999.
View at: Publisher Site | Google Scholar
U. Erben, C. Loddenkemper, K. Doerfel et al., “A guide to histomorphological evaluation of intestinal inflammation in mouse models,” International Journal of Clinical and Experimental Pathology, vol. 7, no. 8, pp. 4557–4576, 2014.
View at: Google Scholar
M. R. Saban, H. Hellmich, N. B. Nguyen, J. Winston, T. G. Hammond, and R. Saban, “Time course of LPS-induced gene expression in a mouse model of genitourinary inflammation,” Physiological Genomics, vol. 5, no. 3, pp. 147–160, 2001.
View at: Publisher Site | Google Scholar
M. R. Dillingh, E. P. van Poelgeest, K. E. Malone et al., “Characterization of inflammation and immune cell modulation induced by low-dose LPS administration to healthy volunteers,” Journal of Inflammation, vol. 11, no. 1, p. 28, 2014.
View at: Publisher Site | Google Scholar
R. A. Luz, P. Xavier-Elsas, B. de Luca et al., “5-Lipoxygenase-dependent recruitment of neutrophils and macrophages by eotaxin-stimulated murine eosinophils,” Mediators of Inflammation, vol. 2014, Article ID 102160, 13 pages, 2014.
View at: Publisher Site | Google Scholar
M. Derouet, L. Thomas, A. Cross, R. J. Moots, and S. W. Edwards, “Granulocyte macrophage colony-stimulating factor signaling and proteasome inhibition delay neutrophil apoptosis by increasing the stability of Mcl-1,” The Journal of Biological Chemistry, vol. 279, no. 26, pp. 26915–26921, 2004.
View at: Publisher Site | Google Scholar
J. M. Williams, C. A. Duckworth, M. D. Burkitt, A. J. M. Watson, B. J. Campbell, and D. M. Pritchard, “Epithelial cell shedding and barrier function,” Veterinary Pathology, vol. 52, no. 3, pp. 445–455, 2015.
View at: Publisher Site | Google Scholar
M. W. Bernart, J. H. Cardellina, M. S. Balaschak, M. R. Alexander, R. H. Shoemaker, and M. R. Boyd, “Cytotoxic falcarinol oxylipins from Dendropanax arboreus,” Journal of Natural Products, vol. 59, no. 8, pp. 748–753, 1996.
View at: Publisher Site | Google Scholar
L. P. Christensen, W. Vach, J. Ritskes-Hoitinga, and K. Brandt, “Inhibitory effects of feeding with carrots or (−)-falcarinol on development of azoxymethane-induced preneoplastic lesions in the rat colon,” Journal of Agricultural and Food Chemistry, vol. 53, no. 5, pp. 1823–1827, 2005.
View at: Publisher Site | Google Scholar
L.-P. Jiang, Y. Lu, B.-M. Nie, and H.-Z. Chen, “Antiproliferative effect of panaxynol on RASMCs via inhibition of ERK1/2 and CREB,” Chemico-Biological Interactions, vol. 171, no. 3, pp. 348–354, 2008.
View at: Publisher Site | Google Scholar
Z. Yan, R. Yang, Y. Jiang et al., “Induction of apoptosis in human promyelocytic leukemia HL60 cells by panaxynol and panaxydol,” Molecules, vol. 16, no. 7, pp. 5561–5573, 2011.
View at: Publisher Site | Google Scholar
K. W. Tan, D. P. Killeen, Y. Li, J. W. Paxton, N. P. Birch, and A. Scheepens, “Dietary polyacetylenes of the falcarinol type are inhibitors of breast cancer resistance protein (BCRP/ABCG2),” European Journal of Pharmacology, vol. 723, pp. 346–352, 2014.
View at: Publisher Site | Google Scholar
Z. R. Haywood Small, “Differential interactions of falcarinol combined with anti-tumour agents on cellular proliferation and apoptosis in human lymphoid leukaemia cell lines,” Journal of Blood Disorders & Transfusion, vol. 6, no. 2, 2015.
View at: Publisher Site | Google Scholar
M. Kobaek-Larsen, R. B. El-Houri, L. P. Christensen, I. Al-Najami, X. Fretté, and G. Baatrup, “Dietary polyacetylenes, falcarinol and falcarindiol, isolated from carrots prevents the formation of neoplastic lesions in the colon of azoxymethane-induced rats,” Food & Function, vol. 8, no. 3, pp. 964–974, 2017.
View at: Publisher Site | Google Scholar
H. T. Le, H. T. Nguyen, H. Y. Min et al., “Panaxynol, a natural Hsp90 inhibitor, effectively targets both lung cancer stem and non-stem cells,” Cancer Letters, vol. 412, pp. 297–307, 2018.
View at: Publisher Site | Google Scholar
S. Bhattacharya, M. K. Rasmussen, L. P. Christensen, J. F. Young, K. Kristiansen, and N. Oksbjerg, “Naringenin and falcarinol stimulate glucose uptake and TBC1D1 phosphorylation in porcine myotube cultures,” Journal of Biochemical and Pharmacological Research, vol. 2, no. 2, pp. 91–98, 2014.
View at: Google Scholar
R. B. El-Houri, D. Kotowska, K. B. Christensen et al., “Polyacetylenes from carrots (Daucus carota) improve glucose uptake in vitro in adipocytes and myotubes,” Food & Function, vol. 6, no. 7, pp. 2135–2144, 2015.
View at: Publisher Site | Google Scholar
S. Purup, E. Larsen, and L. P. Christensen, “Differential effects of falcarinol and related aliphatic C₁₇-polyacetylenes on intestinal cell proliferation,” Journal of Agricultural and Food Chemistry, vol. 57, no. 18, pp. 8290–8296, 2009.
View at: Publisher Site | Google Scholar
S. Kamiloglu, C. Grootaert, E. Capanoglu et al., “Anti-inflammatory potential of black carrot (Daucus carota L.) polyphenols in a co-culture model of intestinal Caco-2 and endothelial EA.hy926 cells,” Molecular Nutrition & Food Research, vol. 61, no. 2, 2017.
View at: Publisher Site | Google Scholar
I.-M. Chung, H. K. Song, S. J. Kim, and H. I. Moon, “Anticomplement activity of polyacetylenes from leaves of Dendropanax morbifera Leveille,” Phytotherapy Research, vol. 25, no. 5, pp. 784–786, 2011.
View at: Publisher Site | Google Scholar
M. M. Czyzewska, L. Chrobok, A. Kania et al., “Dietary acetylenic oxylipin falcarinol differentially modulates GABAA receptors,” Journal of Natural Products, vol. 77, no. 12, pp. 2671–2677, 2014.
View at: Publisher Site | Google Scholar
X. Chi, W. Yao, H. Xia et al., “Elevation of HO-1 expression mitigates intestinal ischemia-reperfusion injury and restores tight junction function in a rat liver transplantation model,” Oxidative Medicine and Cellular Longevity, vol. 2015, 12 pages, 2015.
View at: Publisher Site | Google Scholar
N. Wang, G. Wang, J. Hao et al., “Curcumin ameliorates hydrogen peroxide-induced epithelial barrier disruption by upregulating heme oxygenase-1 expression in human intestinal epithelial cells,” Digestive Diseases and Sciences, vol. 57, no. 7, pp. 1792–1801, 2012.
View at: Publisher Site | Google Scholar
N. Wang, Q. Han, G. Wang et al., “Resveratrol protects oxidative stress-induced intestinal epithelial barrier dysfunction by upregulating heme oxygenase-1 expression,” Digestive Diseases and Sciences, vol. 61, no. 9, pp. 2522–2534, 2016.
View at: Publisher Site | Google Scholar
F. O. Martinez and S. Gordon, “The M1 and M2 paradigm of macrophage activation: time for reassessment,” F1000Prime Reports, vol. 6, 2014.
View at: Publisher Site | Google Scholar
J. Nishihira, M. Sakai, S. Nishi, and Y. Hatanaka, “Identification of the electrophilic substrate-binding site of glutathione S-transferase P by photoaffinity labeling,” European Journal of Biochemistry, vol. 232, no. 1, pp. 106–110, 1995.
View at: Publisher Site | Google Scholar
Y. Zhang, “The molecular basis that unifies the metabolism, cellular uptake and chemopreventive activities of dietary isothiocyanates,” Carcinogenesis, vol. 33, no. 1, pp. 2–9, 2011.
View at: Publisher Site | Google Scholar
Y. Zhang, “Molecular mechanism of rapid cellular accumulation of anticarcinogenic isothiocyanates,” Carcinogenesis, vol. 22, no. 3, pp. 425–431, 2001.
View at: Publisher Site | Google Scholar
H. Yamada, S. Ono, S. Wada et al., “Statuses of food-derived glutathione in intestine, blood, and liver of rat,” npj Science of Food, vol. 2, no. 1, p. 3, 2018.
View at: Publisher Site | Google Scholar
T. Y. Aw, “Biliary glutathione promotes the mucosal metabolism of luminal peroxidized lipids by rat small intestine in vivo,” The Journal of Clinical Investigation, vol. 94, no. 3, pp. 1218–1225, 1994.
View at: Publisher Site | Google Scholar
N. Petri, C. Tannergren, B. Holst et al., “Absorption-metabolism of sulforaphane and quercetin, and regulation of phase II enzymes, in human jejunum in vivo,” Drug Metabolism and Disposition, vol. 31, no. >6, pp. 805–813, 2003.
View at: Publisher Site | Google Scholar
J. Hansen-Moller, S. L. Hansen, L. P. Christensen, L. Jespersen, K. Brandt, and J. Haraldsdottir, Quantification of Polyacetylenes by LC-MS in Human Plasma after Intake of Fresh Carrot Juice, Danish Institute of Agricultural Sciences, 2002.
J. Haraldsdottir, L. Jespersen, J. Hansen-Moller, S. L. Hansen, L. P. Christensen, and K. Brandt, Recent Developments in the Bioavailability of Falcarinol, Danish Institute of Agricultural Sciences, 2002.
Y. Wang, J. Liu, M. Zhu et al., “Biophysical characterization of interactions between falcarinol-type polyacetylenes and human serum albumin via multispectroscopy and molecular docking techniques,” Journal of Luminescence, vol. 200, pp. 111–119, 2018.
View at: Publisher Site | Google Scholar
P. Mehrpouya-Bahrami, K. N. Chitrala, M. S. Ganewatta et al., “Blockade of CB1 cannabinoid receptor alters gut microbiota and attenuates inflammation and diet-induced obesity,” Scientific Reports, vol. 7, no. 1, article 15645, 2017.
View at: Publisher Site | Google Scholar
A. Alhamoruni, K. L. Wright, M. Larvin, and S. E. O'Sullivan, “Cannabinoids mediate opposing effects on inflammation-induced intestinal permeability,” British Journal of Pharmacology, vol. 165, no. 8, pp. 2598–2610, 2012.
View at: Publisher Site | Google Scholar
M. Leonti, L. Casu, S. Raduner et al., “Falcarinol is a covalent cannabinoid CB1 receptor antagonist and induces pro-allergic effects in skin,” Biochemical Pharmacology, vol. 79, no. 12, pp. 1815–1826, 2010.
View at: Publisher Site | Google Scholar

Copyright

Copyright © 2018 Amanda L. Stefanson and Marica Bakovic. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

PDF Download Citation

Download other formats

Order printed copies

Views

4000

Downloads

1533

Citations