Abstract
Dried distillers’ grains with solubles (DDGS)-based diets are nutritious and can improve the inflammations and intestinal immunity in livestock. However, there is limited research examining the effect of feeding DDGS-based diets on changes in intestinal metabolites and related pathways in livestock. In this study, six Guanling crossbred cattle (Guizhou Guanling Yellow cattle × Simmental cattle) were selected and divided into a basal diet (BD) group and an experimental group fed with DDGS replacing 25% of the daily ration concentrates (DDGS) (n=3), respectively. Fresh jejunum (J), ileum (I) and cecum (C) tissues were collected for metabolomic analysis. Differential metabolites and metabolic pathways were explored by means of univariate and multivariate statistical analysis. In comparison to the J-BD group, 123 differential metabolites (VIP > 1, p < 0.05) were identified in the J-DDGS group, which (top 20) were mainly divided into superclasses, including lipids and lipid-like molecules, organic acids and derivatives, and organoheterocyclic compounds. Compared with the I-BD group, 47 differential metabolites were obtained in the I-DDGS group, which were mainly divided into superclasses, including lipids and lipid-like molecules and organic acids and derivatives. The C-DDGS vs. C-BD comparison revealed 88 differential metabolites, which were mainly divided into superclasses, including lipids and lipid-like molecules, organic oxygen compounds, and nucleosides. A total of 34 significant metabolic pathways were found (p < 0.05, −log(p) > 1.3). Among them, 3 significant pathways were significantly enriched in the J-DDGS group, 11 significant pathways were significantly enriched in the I-DDGS group, and 20 significant pathways were significantly enriched in the C-DDGS group. Importantly, primary bile acid biosynthesis, linoleic acid metabolism, and arachidonic acid metabolism correlated with intestinal inflammation and immunity by regulating gut microbiota, prostaglandin synthesis, and cell signaling. The data suggest that DDGS-fed cattle unregulated three metabolic pathways mentioned above and that a DDGS-based diet was able to maintain a balance of these three metabolic pathways, thus resulting in improvement of intestinal inflammation and enhanced immunity in cattle. In conclusion, the DDGS diet has the potential to improve intestinal inflammation and enhance the immunity of Guanling crossbred cattle by regulating the metabolic patterns of lipids and lipid-like molecules, organic acids and derivatives, and related metabolic pathways. These results allude to potential metabolic regulatory mechanisms of DDGS diets and also provide a theoretical basis for the application of DDGS in livestock feed.
1 Introduction
The liquor industry is traditional in China and is also an important economic industry in Guizhou province. Chinese liquor production reached 7.859 million kiloliters in 2019 and produced large numbers of distillers’ grains (DGs) (1). DGs are produced from sorghum, corn, barley, and other pure grains. DGs contain a lot of protein, fat, cellulose, yeast, and enzymes, which are hard for animals to digest and absorb completely. Fresh DGs are perishable (2), and fresh DGs fed directly can easily cause acidosis (3). Therefore, drying fresh DGs to obtain dried distillers’ grains with solubles (DDGS) not only stabilizes the protein content and retains vitamins but also improves the palatability of the feed, prevents mold and acidity from affecting the odor and taste, extends the shelf life, widens the application range and improves the application effect of DGs in animal husbandry (1). Feeding dried DGs has been evidenced to improve the growth performance and meat quality of bulls (4). Current studies on the utilization of DDGS as animal feeds focus on the improvement of animal growth performance, weight gain, milk production in dairy cows, meat quality in beef cattle, antioxidant capacity, and stress reduction (5–9).
The intestine is an important immune-digestive organ of ruminants and is one of the habitats for a large number of microorganisms that play an important role in the energy metabolism of animals and also produce metabolites in direct contact with cells of the intestinal wall (10). The intricate relationship between metabolism and the regulation of immunity and inflammation has been increasingly highlighted in research (11–13). Inflammation is a significant concern in cattle intestines as it disrupts the normal functioning of the intestinal barrier, compromises nutrient absorption, and alters immune homeostasis in cattle (14). Metabolites, which are the small molecules produced during metabolism, have emerged as important mediators in modulating immune responses and inflammatory processes in various organisms (15). Whilst it has been confirmed that these metabolites, resolvins, protectins, and maresins, are generated endogenously by the host, there is an escalating body of evidence that demonstrates intestinal metabolism may produce exclusive mediators that hold biological activity. Certain intestinal metabolites, including essential polyunsaturated fatty acids (PUFAs) such as ω3 and ω6, have been found to significantly impact the host immune system (16). In particular, lipid metabolites derived from ω3-PUFA, such as eicosapentaenoic acid and docosahexaenoic acid, have recently demonstrated potent anti-inflammatory and antiallergenic properties (17). To date, the majority of the studies mentioned have concentrated on regulating the structure and metabolism of intestinal flora in the intestinal contents, with minimal consideration for intestinal wall metabolism. The alteration of indicators in intestinal contents represents, to some extent, the combined effects of bodily function and intestinal microorganisms. However, the metabolic profile of the intestinal wall tends to lean toward signaling alterations in bodily metabolism. We conducted a study to examine the impact of feeding DDGS diets on the intestinal metabolic profile in Guanling crossbred cattle using LC–MS-based non-targeted metabolomic techniques. Our findings offer novel insights into the regulatory effects of dietary DDGS supplementation on intestinal metabolites and their metabolic pathways in ruminants, which could facilitate the future development and utilization of DDGS as a potentially valuable feed resource.
2 Materials and methods
2.1 Origin and treatment of DDGS
The DDGS used in this study were obtained from the Kweichow Moutai Group in Moutai Town, Renhuai, Guizhou, China. The main ingredients of Moutai DGs are distilled sorghum and wheat, which are byproducts of the brewing processes. A drum dryer was used for the drying treatment of the DGs. After centrifugation of fresh Moutai DGs, the filter residues and filtrate were separated, and the filtrate was evaporated and concentrated, and then mixed and dried together with the filter residues to obtain DDGS with a moisture content of 10–15%.
2.2 Animal experiment
This study was conducted at the Yueyawan cattle farm in Guanling County, Anshun City, Guizhou Province (105° 58′ E, 25° 98′ N, altitude, approximately 1863 m). The experimental period was from September 2020 to November 2020, and the average outdoor minimum temperature was 16.9°C and the maximum temperature was 25.6°C. Six Guanling crossbred cattle (Guizhou Guanling Yellow cattle × Simmental cattle) in good health and of similar age (18 months old), weighing 456 ± 26 kg, were provided by the beef cattle fattening farm of Guanling County Yellow Cattle Group. Laboratory tests showed that these cattle were negative for brucella, mycobacterium tuberculosis, foot-and-mouth disease virus, and lumpy skin disease virus infection. Two experimental groups (containing three cattle each) were randomly assigned to one of the two dietary treatments: a basal diet (BD) and a DDGS diet (Jiang-flavor DDGS replaces 25% of the concentrate). The BD was formulated based on the nutritional requirement of 300 kg body weight and 1 kg/d average daily gain according to China’s Beef Feeding Standard (NY/T815-2004), with a forage:concentrate ratio of 60:40 on a dry matter basis. The dietary composition and nutrient levels are shown in Supplementary Tables S1, S2 (17). The cattle were fed at 9:00 and 16:30 every day for 75 days (15 days for adaptive feeding and 60 days for formal feeding of the experimental diet). During the experiment, the cattle drank water freely, and hygiene and daily management were carried out as a matter of routine.
2.3 Collection and preparation of samples
On the 60th day of the formal feeding period, the animals underwent overnight fasting, and then tissues were collected from the jejunum, ileum and cecum, namely, jejunum-BD (J-BD), jejunum-DDGS (J-DDGS), ileum-BD (I-BD), ileum-DDGS (I-DDGS), cecum-BD (C-BD), and cecum-DDGS (C-DDGS). The intestinal sample (intestinal wall) collected in this study refers to the entire thickness of the intestine anatomically including the mucosal layer, submucosal layer, muscle layer, and serosal layer; and it was washed with sterile saline to remove the internal contents. The quality control (QC) samples were obtained by mixing equal volumes of the extracts from all collected samples. Prior to the metabolomics analysis, 30 mg of jejunum, ileum, and cecum tissues were weighed using a JC-TP1203 One Thousandth Electronic Balance (Jingcheng Instrument, Qingdao, China) and transferred into a 1.5-mL tube with two small steel balls. We regarded 20 μL of L-2-chlorophenylalanine (0.3 mg/mL, Hengchuang Biotechnology Co, Shanghai, China) dissolved in methanol (Amperexperiment Technology Co, shanghai, China) as an internal standard. Then 400 μL mixture of methanol/water (1/4, v/v, Amperexperiment Technology Co, Shanghai, China) was added and pre-chilled at −20°C for 2 min and then ground in a grinder for 2 min. The mixtures were subject to ultrasonic separation for 10 min, stored at −20°C for 30 min, and then centrifuged at 13,000 × g for 10 min at 4°C. A total of 300 μL of supernatant was dried in a freeze-concentration centrifugal dryer and resolubilized by 200 μL methanol/water (1/4), then vortexed for 30 s and extracted by ultrasonic for 3 min. After placement for 2 h at −20°C, samples were centrifuged at 4°C (13,000 × g) for 10 min, and 150 μL supernatants were filtered through 0.22 μm microfilters and then transferred to liquid chromatography (LC) vials (18). All chemicals and solvents are analytically pure or of chromatographic grade.
2.4 LC–MS analysis
The LC–MS analysis of jejunum, ileum, and cecum samples in both ESI positive and ESI negative ion modes was performed using the ACQUITY UPLC I Class system (Waters Corporation Milford, USA) coupled with VION IMS QTOF mass spectrometer (Waters Corporation Milford, USA). A 1 μL aliquot of each intestinal tissue sample was injected onto a column ACQUITY UPLC™ BEH C18 (50 mm × 2.1 mm i.d.,1.7 μm; Waters Corporation, Milford, MA, USA). Mobile phase A was 0.1% formic acid in water, and phase B was an acetonitrile/methanol solution (2/3) containing 0.1% formic acid (v/v); the flow rate was 0.4 mL/min. The conditions for UPLC separation and ESI-VIONIMS Q-TOF detection are shown in Supplementary Tables S3, S4. The QC samples were used to evaluate the reproducibility and reliability of the LC–MS system, which contains metabolic information that enables the assessment of the stability of the mass spectrometry system. The ion peaks with a relative standard deviation of >0.4 for the QC group samples were removed, and the stability of the system was evaluated by principal component analysis (PCA). The PCA model plot was obtained after 7 cycles of cross-validation to detect whether the QC samples were closely clustered together, thus judging the stability of the instrument’s detection.
2.5 Data analysis
The original data were processed by the Progenesis QI v2.3 (Nonlinear Dynamics, Newcastle, UK), and metabolites were qualitatively analyzed using the Human Metabolome Database (HMDB), Lipid maps (v2.3), the METLIN database, and a self-created database. For the obtained data, the ion peaks with >50% missing values (0 value) in this group, replacing the 0 value with half of the minimum value, were screened to qualitatively obtain compounds according to the qualitative result evaluation (score). The qualitative results were screened between 36 and 60 points, below which they were considered inaccurate and deleted. Finally, the positive and negative ion data were combined into a data matrix containing all the information extracted from the original data necessary for further analysis. Subsequently, multivariate statistical analyses were carried out using SIMCA 14.0 (Umetrics AB, Umeå, Sweden).
The PCA and orthogonal partial least squares discriminant analysis (OPLS-DA) were performed to reveal the global metabolic changes between the BD and DDGS groups using SIMCA 14.0. An unsupervised PCA was first used to examine both the metabolic differences between the groups and the individual metabolic differences within samples. To maximize the differences between groups within the model, a supervised OPLS-DA was performed on metabolites between groups. In addition, to prevent overfitting of the model, the quality of the model was examined by response permutation testing with 200 responses. Then, univariate analyses were performed on the sample data, which consisted of the student’s t-test and fold change analysis. The fold change (FC) value was calculated through a fold analysis of variance to assess differences in metabolite expression between any two groups. The value of ps were obtained using a student’s t-test, and the volcano plotting was produced using Origin 2020 (Origin Lab, Northampton, MA, USA) to visualize the value of ps and FC values to facilitate rapid identification of metabolites with significant differences. Multivariate and univariate statistical analyses were combined to screen the differential metabolites between groups.
2.6 Key biomarkers and metabolic pathways analysis
To reveal the mechanism of metabolic pathway variation in intestinal samples, an analysis of differential metabolites was carried out with metabolic pathway enrichment analysis based on the Kyoto Encyclopedia of Genes and Genomes (KEGG) database.1 Their KEGG IDs and pathways were obtained, and then the number of metabolites enriched in each corresponding pathway was calculated. The pathway with a value of p < 0.05 was selected as an enriched pathway. The formula for calculating value of ps was as follows:
where N is the total number of metabolites, n is the number of differential metabolites, M is the number of metabolites annotated as a specific pathway, and m is the number of differential metabolites annotated as a specific pathway. A smaller value of p indicates a more pronounced difference within that metabolic pathway.
2.7 Statistical analyses
All continuous variables were expressed as the mean ± standard deviation (M ± SD). The differences between the groups were analyzed using a student’s t-test, where a significant difference was set at p < 0.05. All statistical analyses were performed using SPSS Statistics 26.0 (Chicago, IL, USA).
3 Results
3.1 Quality control of the metabolomic data of the intestinal tissues
LC–MS full-scan detection method was used to illustrate the metabolic alterations in the jejunum, ileum, and cecum tissues from Guanling crossbred cattle fed DDGS diets. A total of 11,028 substance peaks, including 8,464 substance peaks in ESI+ mode and 2,564 substance peaks in ESI− mode, were detectable, and a total of 1,399 metabolites were identified. PCA scoring plots were initially generated using the processed data obtained from metabolomic analysis of the jejunum, ileum, and cecum tissues to evaluate systematic errors in the samples and the trends within each comparison. As shown in Supplementary Figure S1A, the quality control (QC) samples clustered in the center of the PCA score plots, suggesting that the analyses were repeatable and stable. Clear separation trends were observable in the J-DDGS vs. J-BD, I-DDGS vs. I-BD, and C-DDGS vs. C-BD comparisons (Supplementary Figures S1B–D). A tendency for separation on the metabolic spectrum in J-DDGS vs. J-BD, I-DDGS vs. I-BD, and C-DDGS vs. C-BD comparisons was observed in the OPLS-DA score chart (Figures 1A–C). The results of the permutation test strongly indicated that the original model was valid (J-DDGS vs. J-BD: R2 intercept = 0.990, Q2 intercept = 0.452; I-DDGS vs. I-BD: R2 intercept = 0.987, Q2 intercept = 0.670; C-DDGS vs. C-BD: R2 intercept = 0.997, Q2 intercept = 0.845, Figures 1D–F). These results provide assurance for subsequent tests and analyses.
Figure 1
3.2 Differential metabolites in intestinal tissues of DDGS and BD groups
To visualize the results of the fold change (FC) analysis of 1,399 metabolites for quick identification of significantly differential metabolites, a volcano plot was drawn by transferring the FC values of each metabolite to log2 (FC), and by transferring the value of p (p = 0.05) of the student’s t-test to -log (p) and simultaneously meeting the variable importance in projection (VIP) values >1 for the first principal component. As shown in Figures 2A–C, a total of 123 metabolites (103 upregulated with log2(FC) >0 and 20 downregulated with log2(FC) <0), 47 metabolites (28 upregulated and 19 downregulated), and 88 metabolites (9 upregulated and 79 downregulated) were obtained in the J-DDGS group, I-DDGS and C-DDGS groups, respectively.
Figure 2
The levels of the top 50 differential metabolites were visualized by a heat map depicted in Figures 3A–C, in which colors represent increased (red) or decreased (blue) abundance, with the intensity reflecting the corresponding concentration. Of these, the relative richness (referring to the ratio of DDGS/BD) of 23, 4, and 4 metabolites were decreased in the J-DDGS, I-DDGS, and C-DDGS groups, respectively. Conversely, the richness of 3, 12, and 11 metabolites was significantly increased in the aforementioned jejunum, ileum, and cecum comparisons, respectively. Furthermore, the relative richness of 1, 1, and 5 metabolites had no alteration in the aforementioned comparisons.
Figure 3
The classification of the top 20 significantly differential metabolites based on volcano plot and heat map results are shown in Figures 4A–F, with Table 1 providing detailed information. Of these, in the J-DDGS vs. J-BD comparison, they were mainly classified into lipids and lipid-like molecules (5 steroids and steroid derivatives, 9 glycerophospholipids, 2 fatty acyls, and 1 sterol lipid), organic acids and derivatives (1 carboxylic acid and derivatives), and organoheterocyclic compounds (1 pyridine and derivatives). As for the ileum, the differential metabolites of the I-DDGS vs. I-BD comparison were mainly classified into lipids and lipid-like molecules (3 glycerophospholipids, 7 fatty acyls, 2 prenol lipids and 2 steroids and steroid derivatives) and organic acids and derivatives (1 carboxylic acid and derivatives). For the cecum, the differential metabolites of the C-DDGS vs. C-BD comparison were mainly classified into lipids and lipid-like molecules (13 glycerophospholipids and 4 fatty acyls), organic oxygen compounds (1 organooxygen compound), and nucleosides (1 purine nucleosides). Collectively, these results indicate the jejunum, ileum, and cecum metabolite profiles are primarily influenced by DDGS diets.
Figure 4
Table 1
| Metabolites | Formula | m/z | Retention time (min) | Ion mode | VIPa | p-valuesb | Log2(FC)c |
|---|---|---|---|---|---|---|---|
| J-DDGS vs. J-BD | |||||||
| Tauroursodeoxycholic acid | C26H45NO6S | 498.2892 | 6.4239 | Negative | 32.2631 | 0.0486 | 5.3312 |
| Chenodeoxycholic acid glycine conjugate | C26H43NO5 | 448.3065 | 6.5271 | Negative | 15.9113 | 0.0388 | 4.1098 |
| LysoPC (15:0) | C23H48NO7P | 480.3090 | 8.3475 | Negative | 15.2526 | 0.0139 | 1.8735 |
| Glycocholic acid | C26H43NO6 | 466.3164 | 6.1023 | Positive | 10.6080\ | 0.0020 | 2.7012 |
| Taurocholic acid | C26H45NO7S | 498.2884 | 5.9180 | Positive | 10.3656 | 0.0152 | 5.1614 |
| N-docosahexaenoyl GABA | C26H39NO3 | 414.3001 | 6.7901 | Positive | 8.0995 | 0.0406 | 4.4564 |
| PE (16:0/0:0) | C21H44NO7P | 452.2781 | 7.6887 | Negative | 7.0858 | 0.0242 | 1.9801 |
| PE (P-16:0/0:0) | C21H44NO6P | 436.2830 | 7.8675 | Negative | 6.3084 | 0.0261 | 2.4714 |
| CPA (18:0) | C21H41O6P | 438.2978 | 8.3146 | Positive | 5.0802 | 0.0492 | 2.0260 |
| 5beta-Cyprinolsulfate | C27H48O8S | 531.2996 | 6.3824 | Negative | 4.0242 | 0.0098 | 5.5067 |
| N-oleoyl histidine | C24H41N3O3 | 464.3127 | 7.9913 | Negative | 3.3079 | 0.0405 | 2.00561 |
| Eicosapentaenoic acid | C20H30O2 | 303.2316 | 8.1219 | Positive | 2.8704 | 0.0416 | −0.9064 |
| PE (16:1(9Z)/0:0) | C21H42NO7P | 450.2626 | 7.1999 | Negative | 1.8776 | 0.0481 | 1.8110 |
| PC (O-14:1(1E)/0:0) | C22H46NO6P | 450.2983 | 7.4406 | Negative | 1.8724 | 0.0238 | 2.6164 |
| Spongipregnoloside A | C33H52O11 | 623.3431 | 7.7093 | Negative | 1.7392 | 0.0354 | 1.5054 |
| Sodium taurocholate | C26H44NNaO7S | 582.2721 | 5.7792 | Negative | 1.6224 | 0.0036 | 2.2189 |
| PI (19:1(9Z)/22:2(13Z, 16Z)) | C50H91O13P | 951.5941 | 5.9168 | Negative | 1.5179 | 0.0007 | 3.1835 |
| Niacinamide | C6H6N2O | 123.0549 | 0.9748 | Positive | 1.5125 | 0.0394 | −0.7562 |
| PS (18:0/0:0) | C24H48NO9P | 546.2809 | 7.8262 | Negative | 1.4836 | 0.0348 | 1.2241 |
| PC (15:0/20:3(5Z, 8Z, 11Z)) | C43H80NO8P | 814.5612 | 7.7025 | Negative | 1.4395 | 0.0129 | 1.0551 |
| I-DDGS vs. I-BD | |||||||
| PE (18:1(9Z)/0:0) | C23H46NO7P | 480.3085 | 8.2732 | Positive | 8.9231 | 0.0250 | −2.3181 |
| Ornithokinin | C48H77N15O11 | 520.8031 | 4.2282 | Positive | 7.3695 | 0.0201 | −1.6263 |
| 6-Keto-prostaglandin F1a | C20H34O6 | 369.2278 | 5.4216 | Negative | 3.5467 | 0.0018 | 3.5957 |
| L-Arginine | C6H14N4O2 | 175.1186 | 0.6238 | Positive | 3.1896 | 0.0089 | −0.9584 |
| PC (13:0/0:0) | C21H44NO7P | 454.2928 | 8.1150 | Positive | 3.1868 | 0.0389 | −2.0910 |
| Stearoylcarnitine | C25H49NO4 | 428.3734 | 7.9795 | Positive | 2.3794 | 0.0450 | 1.4324 |
| PS (17:0/22:1(11Z)) | C45H86NO10P | 830.5913 | 11.5799 | Negative | 2.2683 | 0.0212 | −0.4616 |
| 20-oxo-heneicosanoic acid | C21H40O3 | 341.3044 | 8.8580 | Positive | 2.1972 | 0.0128 | −1.8547 |
| 9-OxoODE | C18H30O3 | 277.2159 | 8.0256 | Positive | 1.8338 | 0.0416 | −1.5293 |
| Heneicosanedioic acid | C21H40O4 | 339.2893 | 8.2732 | Positive | 1.6711 | 0.0118 | −2.4269 |
| Thromboxane B2 | C20H34O6 | 353.2322 | 5.5398 | Positive | 1.4171 | 0.0263 | 2.6628 |
| 5-(1-hydroxypropan-2-yl) isolongifol-5-ene | C18H30O | 263.2368 | 9.0485 | Positive | 1.3218 | 0.0376 | −2.5925 |
| S-(4-Methylthiobutylthiohydroximoyl)-L-cysteine | C8H16N2O3S2 | 235.0564 | 0.6031 | Positive | 1.2965 | 0.0238 | −0.9712 |
| Ecabet | C20H28O5S | 379.1577 | 8.7462 | Negative | 1.2668 | 0.0075 | −1.3262 |
| 5beta-Cholestane-3alpha,7alpha,24,26-tetrol | C27H48O4 | 454.3891 | 8.0256 | Positive | 1.2047 | 0.0192 | 1.4576 |
| Prostaglandin J2 | C20H30O4 | 317.2107 | 5.5398 | Postive | 1.1707 | 0.0284 | 2.9054 |
| 3b,16a-Dihydroxyandrostenone sulfate | C19H28O6S | 385.1674 | 9.1105 | Positive | 1.0291 | 0.0025 | −3.3290 |
| C-DDGS vs. C-BD | |||||||
| LysoPC (15:0) | C23H48NO7P | 480.3090 | 8.3475 | Negative | 15.1675 | 0.0169 | −2.4709 |
| PE (18:1(9Z)/0:0) | C23H46NO7P | 480.3085 | 8.2732 | Positive | 12.6200 | 0.0337 | −2.0644 |
| PE (16:0/0:0) | C21H44NO7P | 452.2781 | 7.6887 | Negative | 5.7268 | 0.0171 | −2.4957 |
| PE (P-16:0/0:0) | C21H44NO6P | 436.2829 | 7.8675 | Negative | 4.7338 | 0.0407 | −1.9767 |
| PC (P-15:0/0:0) | C23H48NO6P | 464.3139 | 8.5193 | Negative | 4.6287 | 0.0267 | −2.2409 |
| PC (13:0/0:0) | C21H44NO7P | 454.2928 | 8.1150 | Positive | 4.4824 | 0.0256 | −2.3107 |
| CPA (18:0) | C21H41O6P | 438.2978 | 8.3146 | Positive | 3.5690 | 0.0490 | −1.4364 |
| PE (18:2(9Z,12Z)/0:0) | C23H44NO7P | 476.2782 | 7.3993 | Negative | 2.9291 | 0.0456 | −1.7521 |
| N-oleoyl histidine | C24H41N3O3 | 464.3127 | 7.9913 | Negative | 2.6850 | 0.0092 | −1.9593 |
| PS (18:0/0:0) | C24H48NO9P | 546.2809 | 7.8262 | Negative | 2.0920 | 0.0153 | −2.1028 |
| PC (O-11:1(10E)/2:0) | C21H42NO7P | 452.2776 | 7.9657 | Positive | 1.7919 | 0.0202 | −2.6395 |
| PE (16:1(9Z)/0:0) | C21H42NO7P | 450.2625 | 7.1998 | Negative | 1.7826 | 0.0102 | −1.8965 |
| N-stearoyl histidine | C24H43N3O3 | 466.3275 | 8.5674 | Negative | 1.7181 | 0.0234 | −2.5048 |
| PI (17:0/0:0) | C26H51O12P | 631.3092 | 8.3405 | Negative | 1.7167 | 0.0198 | −2.0960 |
| 1,2,10-Trihydroxydihydro-trans-linalyl oxide 7-O-beta-D-glucopyranoside | C16H30O10 | 403.1578 | 8.6431 | Negative | 1.5055 | 0.0497 | −1.5341 |
| Arachidonic acid | C20H32O2 | 303.2323 | 8.6431 | Negative | 1.3587 | 0.0065 | −1.3843 |
| PE (18:1(11Z)/18:1(11Z)) | C41H78NO8P | 742.5400 | 6.0179 | Negative | 1.1811 | 0.0391 | −0.4565 |
| Xanthosine | C10H12N4O6 | 283.0678 | 2.5247 | Negative | 1.1507 | 0.0044 | −1.3721 |
| 9,10,13-TriHOME | C18H34O5 | 329.2331 | 6.0797 | Negative | 1.0758 | 0.0475 | −0.8254 |
| N-(3-trifluoromethylphenyl)piperazine (TFMPP) | C11H13F3N2 | 251.0776 | 2.35975 | Negative | 1.0406 | 0.0207 | −2.9114 |
TOP 20 differential metabolites in different intestinal walls of DDGS-fed Guanling crossbred cattle.
BD, basal diet group, DDGS: mixed diet group containing 25% DDGS derived from Moutai-flavored DG. J, jejunum; I, ileum; C, cecum. aVIP was obtained from the OPLS-DA model, bp was calculated by student’s t-test analysis, p < 0.05, cLog2(FC) indicates the ratio of the average expression of metabolites in the two groups of samples, with positive values indicating upregulation and negative values indicating downregulation.
3.3 KEGG pathway analysis
Next, we investigated which metabolic pathways may be behind the observed intestinal metabolic profile changes associated with DDGS diets. The identified differential metabolites were annotated with KEGG and HMDB. In this study, a total of 34 significant metabolic pathways were identified (p < 0.05, −log(p) > 1.3). Among them, there were 3 significant pathways, namely, primary bile acid biosynthesis, cholesterol metabolism, and choline metabolism in cancer, that were significantly enriched in the J-DDGS group; there were 11 significant pathways (including arachidonic acid metabolism, mTOR signaling pathway, and D-arginine and D-ornithine metabolism, etc.) that were significantly enriched in the I-DDGS group; and there were 20 significant pathways (including linoleic acid metabolism, GnRH signaling pathway, and leishmaniasis, etc.) that were significantly enriched in the C-DDGS group (Figures 5A–C). The detailed information is shown in Table 2. Furthermore, three metabolic pathways, namely, primary bile acid biosynthesis, linoleic acid metabolism, and arachidonic acid metabolism, were found to be linked to intestinal inflammation and immunity. Among them, the primary bile acid biosynthesis and arachidonic acid metabolism metabolic pathways were specific to the jejunum and ileum, respectively. While the linoleic acid metabolism metabolic pathway was shared in the ileum and cecum.
Figure 5
Table 2
| ID annotation | Annotation | In set | −log(p) | FDR | p-values |
|---|---|---|---|---|---|
| J-DDGS vs. J-BD | |||||
| bta00120 | Primary bile acid biosynthesis | 4 | 5.3348 | 0.0000 | 0.000 |
| bta04979 | Cholesterol metabolism | 1 | 1.7150 | 0.1060 | 0.0193 |
| bta05231 | Choline metabolism in cancer | 1 | 1.5208 | 0.1106 | 0.0301 |
| I-DDGS vs. I-BD | |||||
| bta00590 | Arachidonic acid metabolism | 3 | 3.9398 | 0.0016 | 0.0001 |
| bta04150 | mTOR signaling pathway | 1 | 2.2109 | 0.0430 | 0.0062 |
| bta05142 | Chagas disease | 1 | 2.0353 | 0.0430 | 0.0092 |
| bta00472 | D-arginine and D-ornithine metabolism | 1 | 1.7734 | 0.0499 | 0.0169 |
| bta05146 | Amoebiasis | 1 | 1.7014 | 0.0499 | 0.0199 |
| bta05014 | Amyotrophic lateral sclerosis | 1 | 1.6695 | 0.0499 | 0.0214 |
| bta00220 | Arginine biosynthesis | 1 | 1.4563 | 0.0578 | 0.0350 |
| bta05022 | Pathways of neurodegeneration – multiple diseases | 1 | 1.3722 | 0.0578 | 0.0424 |
| bta00591 | Linoleic acid metabolism | 1 | 1.3722 | 0.0578 | 0.0424 |
| bta04974 | Protein digestion and absorption | 1 | 1.3572 | 0.0578 | 0.0440 |
| bta05230 | Central carbon metabolism in cancer | 1 | 1.3428 | 0.0578 | 0.0454 |
| C-DDGS vs. C-BD | |||||
| bta00591 | Linoleic acid metabolism | 2 | 3.3700 | 0.0317 | 0.0004 |
| bta04912 | GnRH signaling pathway | 1 | 2.1319 | 0.0317 | 0.0074 |
| bta05140 | Leishmaniasis | 1 | 2.1319 | 0.0317 | 0.0074 |
| bta04666 | Fc gamma R-mediated phagocytosis | 1 | 2.0073 | 0.0317 | 0.0098 |
| bta04217 | Necroptosis | 1 | 1.9564 | 0.0317 | 0.0111 |
| bta04730 | Long-term depression | 1 | 1.9564 | 0.0317 | 0.0111 |
| bta04664 | Fc epsilon RI signaling pathway | 1 | 1.8696 | 0.0317 | 0.0135 |
| bta05231 | Choline metabolism in cancer | 1 | 1.8696 | 0.0317 | 0.0135 |
| bta04921 | Oxytocin signaling pathway | 1 | 1.8321 | 0.0317 | 0.0147 |
| bta04270 | Vascular smooth muscle contraction | 1 | 1.7975 | 0.0317 | 0.0159 |
| bta05146 | Amoebiasis | 1 | 1.7975 | 0.0317 | 0.0159 |
| bta04611 | Platelet activation | 1 | 1.7655 | 0.0317 | 0.0172 |
| bta04923 | Regulation of lipolysis in adipocytes | 1 | 1.7655 | 0.0357 | 0.0172 |
| bta04726 | Serotonergic synapse | 1 | 1.6818 | 0.0358 | 0.0208 |
| bta04723 | Retrograde endocannabinoid signaling | 1 | 1.6339 | 0.0358 | 0.0232 |
| bta04913 | Ovarian steroidogenesis | 1 | 1.6118 | 0.0358 | 0.0244 |
| bta04925 | Aldosterone synthesis and secretion | 1 | 1.5908 | 0.0358 | 0.0257 |
| bta00232 | Caffeine metabolism | 1 | 1.5708 | 0.0409 | 0.0269 |
| bta04216 | Ferroptosis | 1 | 1.4829 | 0.0409 | 0.0330 |
| bta04750 | Inflammatory mediator regulation of TRP channels | 1 | 1.4673 | 0.0317 | 0.0341 |
The list of metabolic pathways with significant differences in the DDGS group compared to the BD group.
Based on the selection threshold of −log(p) > 1.3 and p < 0.05, 3 significant target pathways were obtained. In set means the number of differential metabolites involved in this pathway; the p-value is calculated from the enrichment analysis; FDR value is the false discovery rate to adjust the p-values.
4 Discussion
Kweichow Moutai liquor is a world-famous Jiang-flavor Baijiu with excellent and numerous fermentation microorganisms. It produces large numbers of nutrient-rich DGs (18). Improper disposal of fresh DGs easily causes waste of resources and environmental pollution, including soil contamination. Reasonable reuse of DGs as feed resources in livestock production is necessary (19). Drying DGs to obtain DDGS is a common strategy for reuse of DGs. Studies have shown that feeding dried DGs can effectively improve the growth performance, slaughter performance, and intestinal development of bulls and other ruminants, making DDGS suitable for available feed resources (20–22). Dried DGs as animal feed additives do not cause alcohol intoxication in animals. Much of the current research revolves around the effect of feeding DDGS diets on the structural metabolism of gut flora in pigs and small animals (23–28). Nevertheless, there is a paucity of reports on the effect of feeding DDGS diets on gut tissue metabolism in ruminants such as cattle. In this study, it was found that the intestinal metabolomic profile of Guanling crossbred cattle fed a DDGS diet differed significantly from those fed a BD diet. The DDGS diet was shown to influence several intestinal metabolic pathways, such as primary bile acid biosynthesis, linoleic acid metabolism, and arachidonic acid metabolism. These pathways are known to be linked to intestinal immunity and inflammation. This implies that the DDGS diet has the potential to positively function in enhancing immunity and improving intestinal inflammation in cattle.
Primary bile acid biosynthesis is a metabolic pathway that is significantly enriched in the jejunum of the DDGS group. Notable metabolites in this pathway include 5beta-cyprinolsulfate, chenodeoxycholic acid glycine conjugate, glycocholic acid, and taurocholic acid, all of which showed significant upregulation in the J-DDGS group (Figure 5A). During primary bile acid biosynthesis, bile acid is synthesized in the liver using bile acid synthase (CYP7A1). This process forms glycocholic acid with glycine, which facilitates the digestion and absorption of fats by emulsifying them and dispersing them in aqueous solution (29, 30). Taurocholic acid, resulting from the fusion of bile acid and taurine, is capable of linking with fats and creating bile salt-fatty acid complexes. This, in turn, promotes the breakdown and absorption of fat while also halting fat build-up in the intestine (31). Synthesized by the enzyme-catalyzed reaction of normal bile acids with sulfuric acid, 5-beta-cyprinolsulphate is a bioactive component of fish oil with antioxidant and anti-inflammatory properties, as well as being capable of regulating the balance of intestinal flora (32). Chenodeoxycholic acid-glycine conjugate is formed by the combination of bile ketone acid (produced by the carboxylation of bile acids in the liver) and glycine, which promotes bile secretion and thus increases fat emulsification and absorption (33, 34). This study and a previously published manuscript (18) suggest that the DDGS diet may promote intestinal fat emulsification and absorption by upregulating the levels of 5beta-cyprinolsulfate, chenodeoxycholic acid-glycine conjugate, glycocholic acid, and taurocholic acid, and by reducing the number of harmful bacteria and increasing the number of beneficial bacteria, thereby improving intestinal health. However, more research is needed to understand these effects.
Arachidonic acid metabolism is ileum-specific, and 6-Keto-prostaglandin F1a, prostaglandin J2, and thromboxane B2 (prostaglandin analogs) are end-products of this pathway, which were markedly upregulated in the I-DDGS group (Figure 5B). 6-Keto-prostaglandin F1a is formed through the metabolic conversion of PGE1 in vivo, which reduces intestinal mucosal damage and relieves gastrointestinal ulcers, as well as having anti-platelet aggregation and anti-inflammatory effects (35–37). Prostaglandin J2 is a substance that is enzymatically converted from prostaglandin H2 (PGH2) or other prostaglandin components by enzymatic action and can promote apoptosis by regulating the production of inflammatory mediators (38, 39). Thromboxane B2 is a platelet-aggregating hormone, a stable metabolite of thromboxane A2 produced through the catalytic reaction of cyclooxygenase and thromboxane synthetase, which has the effect of regulating blood flow, maintaining vascular function, and platelet aggregation (40, 41). Our study showed that feeding DDGS diets exerted a protective effect on the intestine by upregulating the levels of 6-Keto-prostaglandin F1a and prostaglandin J2, which helped maintain the integrity and health of the intestinal mucosa and inhibited intestinal inflammation and tumor cell growth. Upregulation of thromboxane B2 levels may have a negative effect on intestinal blood flow and vascular function. However, more research is needed to understand its specific effects.
Linoleic acid metabolism is shared by the ileum and cecum. 9-OxoODE, 9,10,13-TriHOME, and arachidonic acid are all secondary metabolites in the linoleic acid metabolism, significantly downregulated in I-DDGS and C-DDGS groups. Linoleic acid metabolites are involved in regulating several aspects of the inflammatory process. Among them, 9-OxoODE and 9,10,13-TriHOME are pro-inflammatory and are produced through lipoxygenase-catalyzed linoleic acid metabolism, which can influence the production of inflammatory mediators, such as pro-inflammatory cytokines and leukocyte chemokines (42, 43). Arachidonic acid is a polyunsaturated fatty acid, which is metabolized mainly through the tapping pathway enzymes that catalyze cyclooxygenase and lipoxygenase into metabolites with a variety of biological activities; these metabolites are involved in the genesis and regulation of intestinal inflammation, and reducing their production helps to inhibit the inflammatory process (44, 45). Our study demonstrated that DDGS diets were able to attenuate intestinal inflammation and reduce inflammatory mediators by downregulating the concentrations of 9-OxoODE, 9,10,13-TriHOME, and arachidonic acid, thereby reducing the severity of the inflammatory response. Notably, the effects of linoleic acid metabolites may vary depending on the type and concentration of the particular compound. Further studies are needed to more accurately understand the specific mechanisms of action of linoleic acid metabolites in intestinal inflammation and immunomodulation.
5 Conclusion
Taken together, our findings suggest that implementing a DDGS diet can encourage the production of primary bile acids and promote arachidonic acid metabolism. This is achieved by increasing levels of 5beta-cyprinolsulfate, chenodeoxycholic acid glycine conjugate, glycocholic acid, and taurocholic acid, as well as 6-Keto-prostaglandin F1a, prostaglandin J2, and thromboxane B2 (prostaglandin analogs). Additionally, the levels of 9-OxoODE, 9,10,13-TriHOME, and arachidonic acid inhibition of linoleic acid metabolism are reduced by this diet. The equilibrium of three metabolic pathways sustains a proportional level of intestinal inflammation and immune function, fostering gut inflammation and immunity in Guanling crossbred cattle. Nonetheless, this is solely a preliminary investigation, and extensive analysis with a vast number of animals is necessary to verify the particular regulatory roles and their underlying mechanisms. This study enhances our comprehension of the nutritional and metabolic effects of DDGS diets on Guanling crossbred cattle and sheds light on their underlying mechanisms. Additionally, it provides valuable references for the use of DDGS as a feed for animals.
Statements
Data availability statement
The original contributions presented in the study are included in the article/Supplementary material, further inquiries can be directed to the corresponding authors.
Ethics statement
The animal studies were approved by EAE-GZu-2020-E018, 2 September 2020. The studies were conducted in accordance with the local legislation and institutional requirements. Written informed consent was obtained from the owners for the participation of their animals in this study.
Author contributions
XL, EZ, ZeC, and CC conceived the study. XL, TZ, DX, and MZ performed the experiments. XL, JZ, RZ, GH, EZ, ZhC, and CC analyzed experimental results and data. GH, BZ, KW, CC, and SM assisted with animal experiments. XL wrote the manuscript. All authors have read and agreed to the published version of the manuscript.
Funding
This research was supported by grants from the Guizhou Provincial Department of Agriculture project (No. [2022] 163), the Guizhou Provincial Support Fund of Science and Technology (No. [2021]5646), the Guizhou Provincial Science and Technology Projects (QKHJC-ZK [2022] YB158), the Cultivating Project of Guizhou University (GDPY[2020]85), and the Scientific Research Fund for talents recruiting of Guizhou University (GDRJHZ [2020]63).
Acknowledgments
We kindly acknowledge Kweichow Moutai Group for providing distillers’ grains, and Guizhou Cattle Industry Group Co., Ltd. for providing the Guanling crossbred cattle.
Conflict of interest
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
Publisher’s note
All claims expressed in this article are solely those of the authors and do not necessarily represent those of their affiliated organizations, or those of the publisher, the editors and the reviewers. Any product that may be evaluated in this article, or claim that may be made by its manufacturer, is not guaranteed or endorsed by the publisher.
Supplementary material
The Supplementary material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fvets.2023.1223088/full#supplementary-material
Footnotes
References
1.
LiuYJiangFPengLWuHYouYWangC. Effects of distiller's grains and fermented distiller's grains on rumen fermentation parameters and microflora of simmental hybrid cattle. China Feed. (2022):111–22. doi: 10.15906/j.cnki.cn11-2975/s.20221121
2.
LiuZZhongXYaoYYangF. Biological feed of white distiller's grains and its application status in swine production. Chinese J Anim Nutr. (2020) 32:15–20. doi: 10.3969/j.issn.1006-267x.2020.01.003
3.
WangCWangZSHuRMaJCaoGYaoXHet al. Effects of different types of white distiller’s grains on growth performance, nutrient apparent digestibility, serum biochemical indexes and rumen fermentation parameters of simmental crossbred cattle. Chinese J Anim Nutr. (2021) 33:913–22.
4.
ReisVAReisRAAraujoTLageJFTeixeiraPDGionbelliTet al. Performance, beef quality and expression of lipogenic genes in young bulls fed low-fat dried distillers' grains. Meat Sci. (2020) 160:107962. doi: 10.1016/j.meatsci.2019.107962
5.
LiXHuiYLengBRenJSongYCheLet al. Millet-based supplement restored gut microbial diversity of acute malnourished pigs. PLoS One. (2021) 16:e250423. doi: 10.1371/journal.pone.0250423
6.
DaRESPVilasBESYPaulinoPPaulaSDPossamaiAJDaFLet al. Dried distiller's grains for feedlot Nellore cattle fed non-forage-based diets. Trop Anim Health Prod. (2022) 54:230. doi: 10.1007/s11250-022-03225-4
7.
HubbardKJKononoffPJGehmanAMKelzerJMKargesKGibsonML. Short communication: the effect of feeding high protein distillers dried grains on milk production of Holstein cows. J Dairy Sci. (2009) 92:2911–4. doi: 10.3168/jds.2008-1955
8.
StevensAVKargesKRezamandPLaarmanAHChibisaGE. Production performance and nitrogen metabolism in dairy cows fed supplemental blends of rumen undegradable protein and rumen-protected amino acids in low-compared with high-protein diets containing corn distillers’ grains. J Dairy Sci. (2021) 104:4134–45. doi: 10.3168/jds.2020-19697
9.
YaoKJiangLLiuJWangDLiuHRenD. Effect of yellow wine lees supplementation on milk antioxidant capacity and hematological parameters in lactating cows under heat stress. Animals. (2021) 11:11. doi: 10.3390/ani11092643
10.
NaYRStakenborgMSeokSHMatteoliG. Macrophages in intestinal inflammation and resolution: a potential therapeutic target in IBD. Nat Rev Gastroenterol Hepatol. (2019) 16:531–43. doi: 10.1038/s41575-019-0172-4
11.
Barker-TejedaTCZubeldia-VarelaEObesoD. A step closer to understanding the relationship between host and gut microbiota metabolism. Allergy. (2022) 77:1638–40. doi: 10.1111/all.15246
12.
DingQGaoZChenKZhangQHuSZhaoL. Inflammation-related epigenetic modification: the bridge between immune and metabolism in type 2 diabetes. Front Immunol. (2022) 13:883410. doi: 10.3389/fimmu.2022.883410
13.
LiHWangPZhouYZhaoFGaoXWuCet al. Correlation between intestinal microbiotal imbalance and 5-HT metabolism, immune inflammation in chronic unpredictable mild stress male rats. Genes Brain Behav. (2022) 21:e12806. doi: 10.1111/gbb.12806
14.
LiQYuCChenYLiuSAzevedoPGongJet al. Citral alleviates peptidoglycan-induced inflammation and disruption of barrier functions in porcine intestinal epithelial cells. J Cell Physiol. (2022) 237:1768–79. doi: 10.1002/jcp.30640
15.
OliwEHOkamotoSHornstenLSatoF. Biosynthesis of prostaglandins from 17(18) epoxy-eicosatetraenoic acid, a cytochrome P-450 metabolite of eicosapentaenoic acid. Biochim Biophys Acta. (1992) 1126:261–8. doi: 10.1016/0005-2760(92)90239-r
16.
NagatakeTKunisawaJ. Emerging roles of metabolites of omega3 and omega6 essential fatty acids in the control of intestinal inflammation. Int Immunol. (2019) 31:569–77. doi: 10.1093/intimm/dxy086
17.
BiduCEscoulaQBellengerSSporAGalanMGeisslerAet al. Erratum. The transplantation of omega3 PUFA-altered gut microbiota of fat-1 mice to wild-type littermates prevents obesity and associated metabolic disorders. Diabetes. (2019) 68:235. doi: 10.2337/db19-er01a
18.
SongCZhangTXuDZhuMMeiSZhouBet al. Impact of feeding dried distillers' grains with solubles diet on microbiome and metabolome of ruminal and cecal contents in Guanling yellow cattle. Front Microbiol. (2023) 14:1171563. doi: 10.3389/fmicb.2023.1171563
19.
ZhangJZhangTXuDZhuMLuoXZhangRet al. Plasma metabolomic profiling after feeding dried distiller's grains with solubles in different cattle breeds. Int J Mol Sci. (2023) 24:24. doi: 10.3390/ijms241310677
20.
CorsatoAIDaintonANAldrichCG. A review: nutrition and process attributes of corn in pet foods. Crit Rev Food Sci Nutr. (2022) 62:8567–76. doi: 10.1080/10408398.2021.1931020
21.
CaiFJCaiLYKongBWangJB. Research progress on diversified utilization of distiller's grains. Liquor Making. (2020) 47:11–5. doi: 10.3969/j.issn.1002-8110.2020.02.005
22.
ZhangYX. Feed utilization of distiller's grains and its effect on livestock production and economic benefits. Feed Res. (2021) 44:157–60. doi: 10.13557/j.cnki.issn1002-2813.2021.23.034
23.
SiWJLiuJZHuangDLPengPZhengTKZhaoYPet al. Screening and process optimization of bacteria for fodder utilization of Distiller's grains. Feed Res. (2022) 45:67–72. doi: 10.13557/j.cnki.issn1002-2813.2022.08.015
24.
YuJLXiongQZhangJQWangXLCaiJLHanJXet al. Feed value of corn wet distiller's grains with solubles and concentrated solubles for beef cattle. China Feed. (2023):126–31. doi: 10.15906/j.cnki.cn11-2975/s.2022060042-02
25.
ZenginMSurAIlhanZAzmanMATavsanliHEsenSet al. Effects of fermented distillers' grains with solubles, partially replaced with soybean meal, on performance, blood parameters, meat quality, intestinal flora, and immune response in broiler. Res Vet Sci. (2022) 150:58–64. doi: 10.1016/j.rvsc.2022.06.027
26.
AbudabosAMAl-AtiyatRMAlbatshanHAAljassimRAljumaahMRAlkhulaifiMMet al. Effects of concentration of corn distillers dried grains with solubles and enzyme supplementation on cecal microbiota and performance in broiler chickens. Appl Microbiol Biotechnol. (2017) 101:7017–26. doi: 10.1007/s00253-017-8448-5
27.
ChenHZhangSKimSW. Effects of supplemental xylanase on health of the small intestine in nursery pigs fed diets with corn distillers' dried grains with solubles. J Anim Sci. (2020) 98:98. doi: 10.1093/jas/skaa185
28.
Lopez-GarciaYRGomez-RosalesSAngelesMLJimenez-SeverianoHMerino-GuzmanRTellez-IsaiasG. Effect of the addition of humic substances on morphometric analysis and number of goblet cells in the intestinal mucosa of broiler chickens. Animals. (2023) 13:13. doi: 10.3390/ani13020212
29.
RuanDJiangSQHuYJDingFYFanQLChenFet al. Effects of corn distillers dried grains with solubles on performance, oxidative status, intestinal immunity and meat quality of Chinese yellow broilers. J Anim Physiol Anim Nutr. (2017) 101:1185–93. doi: 10.1111/jpn.12637
30.
ZhongRZXiaJQSunHQinGX. Effects of different sources of protein on the growth performance, blood chemistry and polypeptide profiles in the gastrointestinal tract digesta of newly weaned piglets. J Anim Physiol Anim Nutr. (2017) 101:e312–22. doi: 10.1111/jpn.12607
31.
SongWSParkHMHaJMShinSGParkHGKimJet al. Discovery of glycocholic acid and taurochenodeoxycholic acid as phenotypic biomarkers in cholangiocarcinoma. Sci Rep. (2018) 8:11088. doi: 10.1038/s41598-018-29445-z
32.
OktarBKGulpinarMAErcanFCingiAAlicanIYegenBC. Beneficial effects of glycocholic acid (GCA) on gut mucosal damage in bile duct ligated rats. Inflammation. (2001) 25:311–8. doi: 10.1023/a:1012812616083
33.
XuJXieSChiSZhangSCaoJTanB. Protective effects of taurocholic acid on excessive hepatic lipid accumulation via regulation of bile acid metabolism in grouper. Food Funct. (2022) 13:3050–62. doi: 10.1039/d1fo04085e
34.
SiYCRenCCZhangEWKangZXMoXYLiQQet al. Integrative analysis of the gut microbiota and metabolome in obese mice with electroacupuncture by 16S rRNA gene sequencing and HPLC-MS-based metabolic profiling. Am J Chin Med. (2022) 50:673–90. doi: 10.1142/S0192415X22500276
35.
JiaXSuzukiYNaitoHYettiHKitamoriKHayashiYet al. A possible role of chenodeoxycholic acid and glycine-conjugated bile acids in fibrotic steatohepatitis in a dietary rat model. Dig Dis Sci. (2014) 59:1490–501. doi: 10.1007/s10620-014-3028-3
36.
WalkerSStiehlARaedschRKlotersPKommerellB. Absorption of urso- and chenodeoxycholic acid and their taurine and glycine conjugates in rat jejunum, ileum, and colon. Digestion. (1985) 32:47–52. doi: 10.1159/000199216
37.
VaneJRBottingRM. The mechanism of action of aspirin. Thromb Res. (2003) 110:255–8. doi: 10.1016/s0049-3848(03)00379-7
38.
Figueiredo-PereiraMECorwinCBabichJ. Prostaglandin J2: a potential target for halting inflammation-induced neurodegeneration. Ann N Y Acad Sci. (2016) 1363:125–37. doi: 10.1111/nyas.12987
39.
DosSNIde AquinoTMDaSJE. Computer-aided drug design of anti-inflammatory agents targeting microsomal prostaglandin E (2) synthase-1 (mPGES-1). Curr Med Chem. (2022) 29:5397–419. doi: 10.2174/0929867329666220317122948
40.
FitzGeraldGAPatronoC. The coxibs, selective inhibitors of cyclooxygenase-2. N Engl J Med. (2001) 345:433–42. doi: 10.1056/NEJM200108093450607
41.
WuHLeiZGaoSDaiLHanYGaoHet al. YiqiHuoxue decoction and its ethanol precipitation show anti-platelet and antithrombotic effects by suppressing thromboxane B2 formation. Acta Cardiol Sin. (2019) 35:524–33. doi: 10.6515/ACS.201909_35(5).20190210A
42.
DaCSFGrodzkiAMorganRKZhangZTahaAYLeinPJ. Oxidized linoleic acid metabolites regulate neuronal morphogenesis in vitro. Neurochem Int. (2023) 164:105506. doi: 10.1016/j.neuint.2023.105506
43.
FuchsDTangXJohnssonAKDahlenSEHambergMWheelockCE. Eosinophils synthesize trihydroxyoctadecenoic acids (TriHOMEs) via a 15-lipoxygenase dependent process. Biochim Biophys Acta Mol Cell Biol Lipids. (2020) 1865:158611. doi: 10.1016/j.bbalip.2020.158611
44.
TookerBCKandelSEWorkHMLampeJN. Pseudomonas aeruginosa cytochrome P450 CYP168A1 is a fatty acid hydroxylase that metabolizes arachidonic acid to the vasodilator 19-HETE. J Biol Chem. (2022) 298:101629. doi: 10.1016/j.jbc.2022.101629
45.
DhillonVSDeoPChuaAThomasPFenechM. Telomere length in healthy adults is positively associated with polyunsaturated fatty acids, including arachidonic acid, and negatively with saturated fatty acids. J Gerontol A Biol Sci Med Sci. (2021) 76:3–6. doi: 10.1093/gerona/glaa213
Summary
Keywords
dried distillers’ grains with solubles (DDGS), Guanling crossbred cattle, intestinal wall, metabolite, metabolic pathways
Citation
Luo X, Zhang T, Xu D, Zhu M, Zhang J, Zhang R, He G, Chen Z, Mei S, Zhou B, Wang K, Chen C, Zhu E and Cheng Z (2024) Effect of feeding a dried distillers’ grains with solubles diet on the metabolism of the intestinal wall in Guanling crossbred cattle: a preliminary assessment. Front. Vet. Sci. 10:1223088. doi: 10.3389/fvets.2023.1223088
Received
16 June 2023
Accepted
01 December 2023
Published
09 January 2024
Volume
10 - 2023
Edited by
Massimo Trabalza-Marinucci, University of Perugia, Italy
Reviewed by
Gang Yao, Xinjiang Agricultural University, China; Jon Schoonmaker, Purdue University, United States
Updates
Copyright
© 2024 Luo, Zhang, Xu, Zhu, Zhang, Zhang, He, Chen, Mei, Zhou, Wang, Chen, Zhu and Cheng.
This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Erpeng Zhu, zhu13782701756@126.comZhentao Cheng, ztcheng@gzu.edu.cn
Disclaimer
All claims expressed in this article are solely those of the authors and do not necessarily represent those of their affiliated organizations, or those of the publisher, the editors and the reviewers. Any product that may be evaluated in this article or claim that may be made by its manufacturer is not guaranteed or endorsed by the publisher.