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Effects of different feeding systems on ruminal fermentation, digestibility, methane emissions, and microbiota of Hanwoo steers

  • Seul Lee (Animal Nutrition & Physiology Division, National Institute of Animal Science, Rural Development Administration) ;
  • Jungeun Kim (Animal Nutrition & Physiology Division, National Institute of Animal Science, Rural Development Administration) ;
  • Youlchang Baek (Animal Nutrition & Physiology Division, National Institute of Animal Science, Rural Development Administration) ;
  • Pilnam Seong (Animal Nutrition & Physiology Division, National Institute of Animal Science, Rural Development Administration) ;
  • Jaeyong Song (Nonghyupfeed Inc.) ;
  • Minseok Kim (Division of Animal Science, College of Agriculture and Life Sciences, Chonnam National University) ;
  • Seungha Kang (The University of Queensland Frazer Institute, Faculty of Medicine, University of Queensland)
  • 투고 : 2023.06.18
  • 심사 : 2023.08.04
  • 발행 : 2023.11.30

초록

This study evaluates how different feeding systems impact ruminal fermentation, methane production, and microbiota of Hanwoo steers native to Korea. In a replicated 2 × 2 crossover design over 29 days per period, eight Hanwoo steers (507.1 ± 67.4 kg) were fed twice daily using a separate feeding (SF) system comprising separate concentrate mix and forage or total mixed rations (TMR) in a 15:85 ratio. The TMR-feeding group exhibited a considerable neutral detergent fiber digestibility increase than the SF group. However, ruminal fermentation parameters and methane production did not differ between two feeding strategies. In addition, TMR-fed steers expressed elevated Prevotellaceae family, Christensenellaceae R-7 group, and an unidentified Veillonellaceae family genus abundance in their rumen, whereas SF-fed steers were rich in the Rikenellaceae RC9 gut group, Erysipelotrichaceae UCG-004, and Succinivibrio. Through linear regression modeling, positive correlations were observed between the Shannon Diversity Index and the SF group's dry matter intake and methane production. Although feeding systems do not affect methane production, they can alter ruminal microbes. These results may guide future feeding system investigations or ruminal microbiota manipulations as a methane-mitigation practice examining different feed ingredients.

키워드

INTRODUCTION

Methane gas, a product of anaerobic microbial carbohydrate fermentation in cattle rumen, is second only to carbon dioxide as a prominent greenhouse gas (GHG) impacting global warming [1]. Animal husbandry emissions constitute 16.5% of total GHG emissions, with a continuously increasing global rate [2]. Therefore, developing a methane-mitigation strategy to attenuate ruminant emissions is a worldwide effort and concern. Moreover, the cattle methane conversion factor (MCF) ranges from 2.4% to 9.5% of gross energy intake, depending on diet quality [3]. Thus, reducing enteric methane emissions through dietary methods will ease environmental pressures from beef production and improve cattle efficacy in energy utilization.

Total mixed ration (TMR) is an efficient ruminant feeding system that prevents selective feeding, maintains ruminal pH, and improves carcass yield and quality grade [46]. Alternatively, general or separate feeding (SF) systems provide a concentrate mix with forage through individual feeders [7]. SF accounts for 76.22% of beef production systems in Korea, while the remaining 23.78% are TMR [8]. Previous studies have reported that TMR-fed steers significantly increase enteric methane emission levels and alter ruminal microbial populations, such as Coprococcus and Butyrivibrio, without neutral detergent fiber (NDF) intake changes between TMR and SF groups [7,9]. However, Holstein cattle produce similar methane levels when fed with either TMR or SF [1012]. Although modifying feeding systems can influence enteric methane emission levels without feed additives, further investigation is needed as published results conflict due to varying feed quality, forage-to-concentrate ratio, and particle size. Therefore, feed with the same ingredients must be evaluated through SF and TMR methods for further clarification.

The ruminal microbiome encompasses complex microorganism communities such as archaea, bacteria, fungi, and protozoa [13]. These microbes aid cattle in digestion, provide nutrients, and produce several fermentation products, including methane [14]. Among microbes fermenting feedstuffs in the rumen, bacteria are the most prevalent. Thus, considering methanogen and bacterial populations is imperative when evaluating methane production influences [14], achievable through 16S rRNA gene amplicon sequencing [13,15].

Despite alternative feeding systems being a promising approach for reducing ruminant methane emissions [9], little is known regarding the effects of SF or TMR systems on Hanwoo, beef cattle native to Korea. Therefore, the present study investigates how these two feeding systems (SF and TMR) impact ruminal fermentation characteristics, digestibility, methane emissions, and ruminal microbiota in Hanwoo steers.

MATERIALS AND METHODS

All experimental procedures were approved and performed under the National Institute of Animal Science Institutional Animal Use and Care Committee in Korea guidelines (approval number: NIAS-2018-282). The experiment was conducted in the Livestock Research Building, National Institute of Animal Science, Rural Development Administration in Wanju, Korea.

Animals and experimental design

The crossover design incorporated eight Hanwoo steers with a 507.1 ± 67.4 kg (means ± standard deviation) average initial body weight (BW), approximately 28 months old upon experiment onset. Each experimental period was 29 days long: 14 days in a metabolic cage outside the chamber and 10 days in the chamber for adaptation, and 5 additional days in the chamber for sampling. From Days 15–29, the steers remained inside the chamber all day. Diets were adjusted to 1.5% of the individual BW and consisted of forage and concentrate (F:C = 15:85; dry matter [DM] basis). The steers were randomly assigned to either the SF or TMR group based on BW. SF-group steers were simultaneously fed the concentrate mix and forage in individual feeders. Avoiding selective feeding was not considered, as this experiment mirrored feeding practices at genuine Korean beef farms. TMR feed was obtained using a TMR compounding machine (Horizontal TMR mixer, Daesung ENG, Jeongeup, Korea) with identical feed sources and ratios to SF. A total of 500 kg (as fed) of feed was loaded into the machine and mixed for 10 min. The feed was then dispensed to steers through individual feeders. Table 1 presents all ingredients and chemical compositions of the experimental diets. The animals were fed equal amounts twice daily, at 09:00 and 16:00. Water and mineral blocks were easily accessible.

Table 1. Experimental diet ingredients and chemical compositions

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1)Periods 1 and 2 mean values.

2)Vitamin A, 2,650,000 IU; vitamin D3, 530,000 IU; vitamin E, 1,050 IU; niacin, 10,000 mg; Mn, 4,400 mg; Fe, 13,200 mg; I, 440 mg; Co, 440 mg.

3)Calculated value from 100 – (% of CP + % of EE + % of crude ash + % of aNDF).

DM, dry matter; OM, organic matter; CP, crude protein; EE, ether extract; aNDF, neutral detergent fiber assayed with a heat-stable amylase and residual ash; ADF, acid detergent fiber; NFC, non-fiber carbohydrate; GE, gross energy

Chemical analyses and digestibility

Feed remaining at the end of the day was recorded and collected before morning feeding. Before each period, feed samples were collected and placed in a drying oven at 60℃ for 48 hours. Then, the dried feed samples were ground in a Foss Tecator Cyclotec 1093 Sample Mill (FOSS, Suzhou, China) through a 1-mm screen. The prepared samples were shipped to Cumberland Valley Analytical Services (Waynesboro, PA, USA) for chemical composition analysis. The Association of Official Agricultural Chemists (AOAC) methods [16] were used to analyze DM (#930.15), crude protein (CP; #990.03), acid detergent fiber (ADF; #973.18), ash (#942.05), and calcium and phosphorus (#985.01). Ether extract (EE; #2003.05) was determined using AOAC methods [17]. NDF was analyzed utilizing heat-stable amylase with residual ash (aNDF) [18]. Dry matter intake (DMI) was calculated daily from the as-fed intake of individual steers. CP was calculated by multiplying the nitrogen content by 6.25.

Whole feces were collected daily during the five-day sampling period (Days 25 to 29). Feces were dropped from the caudal region and gathered in an iron plate. After collection, the daily feces were left in a drying oven at 60℃ for 48 hours. The dried samples were pooled, and 200 g of fecal subsamples were collected for the apparent total-tract digestibility analysis. Fecal compositions were analyzed following AOAC methods [19]: CP (#942.05), EE (#920.39), and ash (#954.01). The NDF and ADF contents were analyzed using the method proposed by Van Soest et al. [18], and CP and non-fiber carbohydrate (NFC) contents were calculated as previously described. The apparent digestibility of any given nutrient was calculated from the individual DMI and feces excreted.

Methane gas measurement

Methane emissions from eight Hanwoo steers within each period were measured using four respiratory chambers with two batches of four animals. Each chamber had a volume of 25.4 m3 (3.9 × 2.6 × 2.5 m, L × H × W, Changsung Engineering, Gwangju, Korea), concrete outer walls, and a front door fixed with a transparent window (300 mm × 150 mm) for observation. In addition, a metabolic cage made of steel pipes (1,400 mm × 2,950 mm × 2,120 mm) was fixed within the chamber for keeping animals in one place. Four 24-V air circulation fans were installed at 45° angles on each side of the chamber ceiling for even air circulation. A PVC (Φ100) tube was installed at the center of the ceiling, and an air motor was attached to the PVC end behind the chamber for continuous air exhaust. In addition, three non-woven profiler layers were installed at the air outlet on the front PVC pipe to prevent dust and animal hair from entering the pump. An identical PVC pipe was inserted through the ceiling at the front of the chamber for fresh air flow

Air samples were vented through an infrared methane sensor (Horiba VIA-510 gas analyzer, Horiba, Kyoto, Japan) to measure methane emissions within a 0–200 ppm detectable range (± 0.2 ppm resolution). Furthermore, a dehumidifier (KAFM251-03, KCC, Jeonju, Korea) was installed for more precise methane analysis, and an Oxymax system consisting of an air pump, a flow meter, a sample pump, and a gas drying device (incorporating an Oxymax sample max, system sampling pump, Paramax-101, and carbon dioxide sensor; Columbus Instrument International, Columbus, Ohio, USA) for gas analysis.

A standard methane-recovery rate was performed thrice before the experiment and thrice after to evaluate the accuracy of the four chambers. First, 5 L of methane gas (99.95% purity) was released into the chamber at a 900 L/min rate and measured in five-second intervals until the methane gas concentration in the air discharged from the chamber reached 0 ppm. The average methane gas recovery rate was 92.45% (SD = 9.27), and the recovery rate of each chamber was used to calculate methane emissions after the experiment. Next, airstreams from the chambers were sequenced to an analyzer at five-minute intervals in a 20-minute cycle for each chamber. The sampled gas was stabilized for 4.5 minutes, and the air sample was then quantified for 30 seconds from each chamber to measure the gas levels. Sample stream sequencing to the analyzer was controlled using a CI-Bus serial interface (Columbus Instrument International).

Methane emissions were measured for four consecutive days (Days 25 to 28), and the data generated during 1 hour after feeding (2 hours a day total) were not included in calculations due to interruptions from open doors. Methane generation during the open-door period was estimated through interpolation. After measuring methane emissions at 0900 hours, the doors were opened for approximately 10 minutes to feed the animals, clean the metabolic cage, and check equipment. This process was repeated at 1600 hours. Methane emission calculations considered chamber temperature and relative humidity, wind speed of the air discharged through the main discharge pipe, and analytical gas concentrations (Table 2). The chamber program maintained a 20℃, 50% humidity, and 900 L/min wind speed, and real-time data and methane detection were automatically recorded simultaneously.

Table 2. Equations for methane production conversion [79]

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The average methane emissions of each chamber from Days 25 to 28 were utilized for the statistical analysis. The MCF was determined as the gross energy percentage of feed converted to methane [1]. Similarly, the methane emission factor (MEF; kg of methane/head/year) was determined by the gross energy intake (MJ/head/d) × (MCF ÷ 100) × 365 ÷ 55.65 (MJ/kg of methane) [1].

Rumen sampling and fermentation parameters

Ruminal fluid was collected from each animal before morning feeding on Day 29 with a stomach tube that we previously developed [20]. The stomach tube includes a head segment (length 13 cm, diameter 3 cm), a flexible tube (length 210 cm, diameter 1 cm), and a vacuum pump (Welch & Thomas, Mount Prospect, IL, USA) to obtain the ruminal fluid. The stomach tube was thoroughly washed with warm water between sampling to prevent cross-contamination. Additionally, the first 200 mL of the ruminal fluid was discarded to reduce any contamination from the saliva [21,22]. The sampled ruminal fluid was filtered through a four-layered cheesecloth. A pH meter (Pinnacle pH meter M540, Corning, NY, USA) measured the sampled inoculum pH immediately after collection. Then, the ruminal fluid was sealed in a tube and frozen in liquid nitrogen. The samples were stored at -80℃ until volatile fatty acids (VFA), ammonia nitrogen (NH3-N), and metagenomic DNA extraction were analyzed.

VFA and NH3-N concentrations were determined as described by Erwin et al. [23] and Chaney and Marbach [24] with minor modifications. Briefly, the ruminal fluids were centrifuged at 14,000×g for 10 minutes at 4℃, and 5 mL of the supernatant was mixed with 500 μL of 50% metaphosphoric acid (MPA; Catalog number 239275, Sigma-Aldrich, St. Louis, MP, USA) for VFA or 500 μL of 25% MPA for NH3-N. Then, the mixture was further centrifuged at 14,000×g for 10 minutes at 4℃ for VFA analysis, and the supernatants were distributed to gas chromatograph (GC) analysis vials (6890N, Agilent Technologies, Wilmington, DE, USA) with a capillary column (Nukol™ Fused silica capillary column, 15 m × 0.53 mm × 0.5 µm, Supelco, Bellefonte, PA, USA) and analyzed. Next, the standard curve was generated using a VFA standard solution (Catalog number 46975-U; Sigma-Aldrich). The inoculum and 25% MPA mixtures were centrifuged at 14,000×g for 5 minutes at 4℃ for NH3-N analysis. After centrifugation, 20 μL of the supernatant was mixed with 1 mL of a phenol color reagent (50 g/L of phenol plus 0.25 g/L of nitroferricyanide) and 1 mL of an alkali-hypochlorite reagent (25 g/L of sodium hydroxide and 16.8 mL/L of 4%–6% sodium hypochlorite). Finally, the mixture was colored in a 37℃ water bath for 15 minutes, 8 mL of distilled water was added, and a UV spectrophotometer (Bio-Rad, US/benchmark plus, Tokyo, Japan) measured the NH3-N concentration at 630-nm absorbance. All analyses were conducted thrice, and the mean values were established.

Metagenomic DNA extraction and analysis

Metagenomic DNA was extracted from the ruminal fluid samples collected on Day 29. Frozen samples were thawed at room temperature, and DNA was extracted following the RBB+C bead-beating method [25]. The V3–V4 region of 16S rRNA genes from each DNA sample was amplified with the universal primers 341F (5’-CTACGGGNGGCWGCAG-3’) and 805R (5’-GACTACHVGGGTATCTAATCC-3’) for bacterial analysis [26]. In addition, the V6–V8 region of 16S rRNA genes was amplified using primers 915F (5’-AGGAATTGGCGGGGGAGCAC-3’) and 1386R (5’-GCGGTGT GTGCAAGGAGC-3’) for methanogen analysis [27]. The primer sets produced approximately 450 and 470 base paired-end protocols with the MiSeq platform (Illumina, SanDiego, CA, USA) at the Macrogen Sequencing Facility (Macrogen, Seoul, Korea).

Raw sequences were pre-processed, quality filtered, and analyzed using QIIME2 (version 2019.1), a next-generation microbiome bioinformatics platform, adhering to the developer’s recommendations [28, 29]. The amplicon sequence variants (ASVs) were generated using the DADA2 algorithm [30] to denoise and remove chimeric sequences. Then, a bacterial analysis was accomplished using the “SILVA_132 99% OTUs full-length sequences” database for taxonomic determination and the Rumen and Intestinal Methanogen (RIM)-DB as a reference [31]. Data sets were then transferred and analyzed through various R packages, such as phyloseq [32], vegan [33], Ampivis2 [34], DESeq2 [35], and ggplot2 [36], for relative abundance, microbial diversity matrix, and correlation calculations.

Bioinformatics and statistical analysis

Data were analyzed by the SAS PROC MIXED (Enterprise Guide 7.1, SAS Institute, Cary, NC, USA) for crossover design. Before data analysis, we conducted the normality test by the Shapiro–Wilk test using the XLSTAT statistical software (Addinsoft, New York, NY, USA) and confirmed that the normality assumption was met. The experimental unit was an individual steer, and the fixed effects were period and diet. However, the period effect is not displayed because there were no statistical differences. Data are presented as least-squares means. Significant differences were defined at p < 0.05, and tendencies were determined at 0.05 ≤ p < 0.1.

Statistical microbiome analysis was conducted with various R packages as previously described. Alpha diversity indices, such as Shannon’s index and Chao1, were calculated with the phyloseq R package, and ANOVA test significance. The principal coordinate analysis (PCoA) assessed beta diversity on Bray–Curtis dissimilarity with the ADONIS permutational multivariate analysis. Correlations between the Shannon Index and various factors such as DMI, methane production, and MEF were completed using a linear regression model.

RESULTS

Feed intake, digestibility, and ruminal fermentation

DM and gross energy intake did not vary by the feeding method (p > 0.10; Table 3). The feeding system type did not affect DM, CP, and NFC digestibility (p > 0.10). Although NDF digestibility (NDFD) differed between the feeding groups, the NDFD of the TMR group was 4.73% higher than the SF (p = 0.013).

Table 3. Feeding method effects on nutrient intake and apparent total tract digestibility in Hanwoo steers

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SF, feeding concentrate and forage separately; TMR, total mixed ration; DM, dry matter; CP, crude protein; NDF, neutral detergent fiber; NFC, non-fiber carbohydrate.

Methane production and ruminal fermentation

The different feeding methods did not affect methane production (g/d), DMI (g/d/kg), digestible (d) DM (g/d/kg), dNDF (g/d/kg), or MCF yields (p > 0.10; Table 4). Consequently, the MEF increased and was more elevated in the TMR group than in the SF (p = 0.089). There were no ruminal fermentation parameter differences between the groups (p > 0.05; Table 4).

Table 4. Feeding method effects on methane production, methane conversion factor, methane emission factor, and ruminal fermentation yields in Hanwoo steers

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1)Methane conversion factor = gross energy percent in feed converted to methane [1].

2)Methane emission factor = (MJ/head/d of gross energy intake) × (MCF ÷ 100) × 365 ÷ (55.65 MJ/kg of methane) [1].

SF, separate feeding concentrate and forage; TMR, total mixed ration; DMI, dry matter intake; OMI, organic matter intake; dDMI, digestible dry matter intake; dOMI, digestible organic matter intake; dNDFI, digestible neutral detergent fiber intake.

Ruminal microbiota

Illumina sequencing detected 172,902 bacterial and 140,210 archaeal sequences. Notably, the Shannon Diversity Index of ruminal bacteria was significantly higher in TMR-fed steers (p = 0.038; Fig. 1A), while ruminal archaea levels did not differ between the groups (p = 0.87). The Chao1 Index of both ruminal bacteria and archaea did not significantly differ between the two feeding systems (Fig. 1A). The PCoA plots did not indicate a relationship between feeding methods and ruminal microbes (p > 0.10; Fig. 1B).

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Fig. 1. Bacteria and archaea community diversities. Shannon and Chao1 indices (A) with Wilcoxon signed-rank test and principal coordinate analysis (PCoA) plots (B) on Bray–Curtis dissimilarity with ADONIS permutational multivariate analysis. Samples were collected from Hanwoo steers fed by separated feeding (SF; n = 8) or total mixed ration (TMR; n = 8).

Fig. 2 displays the relative abundance of bacterial phyla and archaeal genera in Hanwoo steer rumens. The most dominant ruminal bacterial phylum in both feeding groups was Bacteroidetes (SF: 57.66%; TMR: 52.03%), followed by Firmicutes (SF: 33.72%; TMR: 34.44%) and Proteobacteria (SF: 8.04%; TMR: 9.06%; Fig. 2A). Bacteroidetes and Firmicutes comprised 80.0%–96.6% of the total taxonomic profile. Fourteen minor phyla were also detected: Fibrobacteres, Patescibacteria, Spirochaetes, Tenericutes (or Mycoplasmatota), Lentisphaerae, Cyanobacteria, Elusimicrobia, Planctomycetes, WPS-2, Verrucomicrobia, Chloroflexi, Kiritimatiellaeota, Actinobacteria, and Synergistetes. The Methanobrevibacter genus was the most prevalent among the ruminal archaeal genera (77.9%–99.3%; Fig. 2B). The other sorted genera included uncultured archaea families Methanobacteriaceae and Methanomethylophilus: Candidatus methanomethylophilus, Methanosphaera, Methanomicrobium, and Methanimicrococcus. However, there were no significantly different bacterial phyla and archaeal genera between the feeding groups.

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Fig. 2. Bacterial phyla (A) and archaeal genera (B) taxonomic profiles expressed as relative abundances. Samples were collected from Hanwoo steers fed by separated feeding (SF; n = 8) or total mixed ration (TMR; n = 8). The term “uncultured” refers to uncultured Methanomethylophilus.

The SF group expressed higher abundances of the Ruminococcaceae family genera (p < 0.05): CAG-352, Ruminococcaceae UCG-014, Ruminococcaceae NK4A214 group, Ruminococcus 2, and Eubacterium coprostanoligenes. Compared to TMR-fed cows, the bacterial abundance of SF group was more enriched with the following genera: gut Rikenellaceae RC9, Lachnospiraceae NK3A20, Erysipelotrichaceae UCG-004, Succinivibrio, Oribacterium, and Moryella (p < 0.05). Comparatively, the TMR group exhibited relatively higher levels of the Prevotellaceae family (genera Prevotellaceae UCG-011 and Prevotella 1) than the SF group (Fig. 3). Moreover, the bacterial abundance of the TMR group included: Lachnospiraceae ND3007, Christensenellaceae R-7, Ruminobacter, Ruminococcus 1, Candidatus saccharimonas, and an unidentified Veillonellaceae family genus (p < 0.05).

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Fig. 3. Bacterial taxa (genus) plot conveying significantly distinctive abundances between groups. Genus-level bacterial abundances diverged considerably between separated feeding (SF; n = 8) and total mixed ration (TMR; n = 8) groups, as detected and filtered by DESeq2. Genera with adjusted p < 0.05 and estimated log2 fold differences were considered significantly differentially abundant and included in the plot. Each point represents a single genus colored at the family level. The size of each point reflects the log10 mean abundances of the taxonomic genus.

A linear regression analysis was conducted between the bacterial or archaeal Shannon Diversity Index and DMI, methane production, and MEF (Fig. 4) (Table 5). Positive bacterial diversity and DMI correlations were noted in the SF group (R2 = 0.448; p = 0.07); however, statistical archaea differences were not observed (p > 0.10; Fig. 4A). The Shannon Diversity Index (bacteria and archaea) and methane production indicated positive correlations in the SF group (Figs. 4B and 4C); bacterial and archaeal diversities had significantly different correlations with methane production in SF-fed steer (R2 = 0.552 and 0.568 and p < 0.05) (Fig. 4B). In addition, the MEF diversity of the SF group regression models exhibited substantial bacteria (R2 = 0.531; p = 0.04) and an archaea tendency (R2 = 0.46; p = 0.064; Fig. 4C). In contrast, no significant differences were observed between bacterial diversity and methane or MEF in the TMR group (p > 0.10).

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Fig. 4. Linear regression modeling. (A) Bacterial and archaeal diversities (Shannon Diversity index) and dry matter intake (DMI), (B) methane production (CH4, g/d), and (C) methane emission factor (MEF) linear regression analyses. Samples were collected from Hanwoo steers fed by separated feeding (SF; n = 8) or total mixed ration (TMR; n = 8). Shaded regions represent 95% confidence intervals.

Table 5. Bacterial and archaeal Shannon Diversity index, dry matter intake, and methane emissions from Hanwoo steers linear regression analyses

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DMI, dry matter intake; SF, separate feeding concentrate and forage; TMR, total mixed ration; CH4, methane; MEF, methane emission factor.

DISCUSSION

Ruminal fermentation, microbiota, and methanogenesis are most impacted by diet, followed by breed, host, and other feeding system factors [7,9,15,37]. However, research on how different feeding systems impact ruminal fermentation and methanogenesis in Hanwoo cattle is severely limited. Therefore, we compared the ruminal fermentation, methane emissions, and microbiota of Hanwoo steers when provided with the same amount of feed through SF or TMR systems. Steers were allowed to express selective feeding to mirror Korean beef farm conditions. Moreover, restricted feeding in which steers can entirely consume feed was chosen to compare the exact methane yields by feeding methods.

Previously reported results on feeding method-induced NDFD are inconsistent. One study identified higher fiber digestibility in TMR-fed Hanwoo steers [38], corroborating similar studies that observed improved NDFD in TMR-fed Holstein steers [39]. However, synonymous results were obtained through different feeding systems [7,9]. The apparent factors influencing NDFD are forage particle size, forage maturity, passage rate, and feed intake [4042]. This study noted that the TMR group exhibited higher NDFD without DMI or ruminal pH fluctuations. Therefore, NDFD alterations may be caused by ruminal bacteria shifts based on the feeding system. Bekele et al. [43] identified Prevotella as the dominant genus in the rumen; many Prevotella members are uncultured and could be involved in fiber degradation. Similarly, the present study revealed that the Prevotellaceae family was abundant in the TMR-diet group, and the presence of unknown Prevotella strains in this family may contribute to fiber degradation, increasing the NDFD of the TMR group. Kononoff et al. [44] indicated that reduction of forage particle size led to increased NDFD. Therefore, the increase in the NDFD in the TMR group may be attributable to the reduction in the particle size during TMR manufacturing. In this study, the improved NDFD in the TMR group could likely be because of the increase in the surface area attacked by the Prevotella species. However, several studies have shown that reduced particle size is associated with decreased fiber digestibility when the increase in the passage rate exceeds that in the digestibility rate [45,46]. In this study, the distribution of feed particle size in the TMR group was > 19 mm (25%), 8–19 mm (25%), and < 8 mm (50%). These particle sizes in the TMR group does not seem to lead to a considerable increase in the passage rate.

In addition, ruminal pH may correlate with methane production; as ruminal pH increased from 5.7 to 6.5, methane production potentially increased as well [47,48]. Crossbred beef heifers’ ruminal pH and methane production associations have been previously reported [49], evidenced by decreased activity of methanogens when ruminal pH is lowered from the dietary concentrate elevation [50]. In this study, the dietary F:C ratios of the SF and TMR group were equally set, demonstrating no changes in the ruminal pH and ruminal methanogen abundance of either group. Thus, methane production may remain unchanged between the treatment groups.

Methane production and MCF between the groups were not significantly different. However, MEF did tend to differ relative to treatment (p = 0.067) because MEF calculations consider gross energy intake and MCF as factors. Previous study results varying from those in this experiment may be due to disproportional forage quantities in the feed. Feed in other studies contained 27% [9] and 25% [7] of roughage as the DM basis; however, in the present study, the feed only contained 15% of roughage. Alterations in the F:C ratio affect the ruminal fermentation environment and determine the feed nutritional levels [51]. The F:C ratio is adjusted relative to the cattle growth stage. The present study selected the F:C ratio for the Hanwoo fattening stage based on Korean feeding standard recommendations [52]. Therefore, in this study, smaller roughage amounts might be responsible for the different results from previous studies.

Furthermore, previous studies have divulged higher methane production and yield in TMR-fed Holstein and Hanwoo steers [7,9]. However, additional studies proclaimed no statistical differences between SF and TMR feeding systems concerning methane emission from Holstein cows [11] and steers [10,12]. Studies that recounted no differences in the methane yield based on feeding methods are consistent with the results of this study. The inconsistent methane production among studies is due to variations in the nutritional level, forage type, and F:C ratio feed. These factors affect ruminal fermentation, subsequently impacting ruminant methane emission [53,54].

The Intergovernmental Panel on Climate Change (IPCC) formed the MEF to estimate methane generated during livestock feed digestion and utilize these findings to establish country-specific emission statistics [1]. Korea has also developed emission factors for beef (Hanwoo) and dairy cattle (Holstein). The Korean ruminant MEF is lower than the IPCC value (over 1-year-old Hanwoo, 61 kg/methane/head/year; IPCC, 64 kg/methane/head/year) because of the country’s unique feeding system [55]. In this study, the MEF was 57.59 in the SF group and 61.18 in the TMR, comparable to the Korean inherent emission factor. Jo et al. [56] analyzed several MEF prediction methods; Hanwoo steers MEF at the finishing stage was predicted as 33.9 when the IPCC Tier 2 method was used. However, Bharanidharan et al. [7] reported that Hanwoo steers MEF measured through respiration chambers was 35.1 in SF and 49.4 in TMR, higher than those predicted by Jo et al. [56] and lower than the measured values in this study. This difference can be explained by experimental animal BWs, which averaged 292 kg in the previous study [7] and 507 kg in this one.

Very few studies have investigated how feeding systems impact ruminant methane emissions. A previous study indicated that an SF diet reduced methane production from Holstein steers even more than the TMR diet did [9]. However, methane production did not differ between TMR and SF strategies in the present study. Bharanidharan et al. [7] elucidated that methane emissions deviated between different breeds fed the same diet (TMR or SF) under identical management conditions. Therefore, this contradictory result is potentially due to breed differences. Yurtseven et al. [57] demonstrated that diet composition impacts methane emissions. Similarly, these contrasting methane production findings could be from varying diet compositions between studies [9]. In a previous study, roughage was fed to animals first, followed by concentrate after 40 minutes [9]; however, avoiding SF was not considered in the present study and may have also contributed to the different production calculations. Thus, the abovementioned factors should be considered in future studies using different feeding systems as a methane-mitigation practice in ruminants.

Although the different feeding practices in this study did not shift prominent microbes, some minor bacterial abundance fluctuations were observed. Ruminal Rikenellaceae have reported a negative relationship with the NDFD, ADFD, and methane yield (L/kg metabolic BW) in sheep [58], corroborating the current study’s findings that the NDFD of the SF group was lower than that of the TMR group. However, Rikenellaceae abundance was also prevalent when yaks were fed fiber-rich diets [59] or when Holstein cows were fed low-starch diets [60]. Erysipelotrichaceae, subsuming the genus Erysipelotrichaceae UCG-004, exhibited a relatively high abundance in sheep rumen with a low methane yield, similar to the present study results where its relative abundance was high in SF with a low MEF [61].

Succinivibrio ferments starch to dextrin in animals [62,63], and some strains possess enzymes that dismantle plant cell walls [64]. Studies using cashew nut shell supplements to attenuate ruminal methane have confirmed reduced methane production or yield with a higher Succinivibrio dextrinosolvens abundance [65,66]. Moreover, previous reports have revealed that lower methane-emitting cows had a higher Succinivibrio spp. ruminal abundance [67,68]. In this study, the SF group did exhibit some bacterial species causing low methane emissions; however, the bacterial community of the TMR group conveyed contradictory results. This observation suggests that methanogens and further bacterial species identifications are required to clarify the methane emission and ruminal microbe relationship.

Prevotellaceae UCG-011 and genus Prevotella 1 ASVs were higher in the TMR group than in the SF group. Prevotellaceaeis is a bacterial family that degrades hemicellulose, pectin, starch, and protein in the rumen [6971]. Despite Prevotella being a prominent bacterium abundant in the rumen, the functions of only some identified species (P. ruminicola and P. bryantii) are known. Although the present study signified that the TMR group with more Prevotellaceae microbes also expressed more MEF, previous studies convey contradictory results. In a cohort study, Colombian buffalos had abundant ruminal Prevotella species in a low methane-emitting group [72]. Moreover, heifers fed with low-forage-containing diets (F:C = 30:70) indicated intensified Prevotella species prevalence [73]; however, Prevotella species dominated high-forage diet-fed cow rumen (F:C = 65:35 and 50:50) compared to low-forage diets (F:C = 35:65) [74]. Another study certified that the Prevotella species was positively correlated with methane yield, NDFD, and ADF digestibility (ADFD) [58], which complements the present study results. These conflicting findings suggest that further studies are required to understand the effect of Prevotellaceae on ruminant methane emissions.

The TMR group, which had a higher NDFD than the SF group, also had relatively higher levels of the Christensenellaceae R-7 genus and the Veillonellaceae family. The Christensenellaceae R-7 group is abundant in high-forage diets and positively correlates with the DMD, NDFD, ADFD, and methane yield [58,59], partially coinciding with our results. The Veillonellaceae family produces propionate as their fermentation end-product. Thus, Veillonellaceae levels are consistently higher in Holstein dry cows fed with high-starch diets [60]. Methane emission was also reduced through encapsulated nitrate supplementation in Nellore steers [68]. A previous study observed Boer goats with a low NDFD [75]. However, Veillonellaceae bacterial family abundance shifts could not be confirmed in this study. Thus, the influence of unidentified ruminal bacteria needs careful investigation.

Although there were no observable statistical DMI and methane emission differences between SF and TMR, the microbial diversity index and DMI, methane production, and MEF linear regression differed by the feeding system. The SF method presented linear regression models applicable for bacteria and archaea approximation; however, none were suitable for the TMR group. Therefore, it is assumed that maintaining a stable ruminal TMR feed environment contributed to maintaining consistent microbial diversity. Previous studies have reported that the TMR systems maintain ruminal pH and acetate-to-propionate ratios, as TMR provides a more balanced and uniform roughage-to-concentrate ratio [76,77].

TMR feeding decreases selective feeding behavior and maintains a stable ruminal environment. Hasty changes in the rumen from the SF strategy can relocate microbes, potentially affecting the DMI and bacterial diversity relationship. However, studies resembling the present experiment did not report a Shannon Diversity Index and DMI correlation [7,9]. Hence, further studies are required to verify the feed intake and bacterial diversity association. Nonetheless, the positive correlation between bacterial diversity, methane production, and MEF is linked to specific bacteria shifts (Fig. 3). Furthermore, an archaeal diversity and methane production association was observed as most ruminal archaea belong to Methanogens [78].

CONCLUSION

This study concluded that different feeding systems for Hanwoo steers given F:C = 15:85 diets did not affect methane production. The overall microbial composition based on the PCoA plot was analogous between feeding systems, although some ruminal microbes did shift. Based on the current data, feed ingredient factors must be considered for further study using different feeding systems to reduce ruminant methane generation. Our results will aid future studies in developing novel feeding systems that reduce methane production by manipulating the ruminal microbiota composition.

참고문헌

  1. IPCC [Intergovernmental Panel on Climate Change]. Summary for policymakers. In: Climate change 2007: mitigation of climate change. Contribution of working group III to the Fourth Assessment Report of the Intergovernmental Panel on Climate Change. New York, NY: Cambridge University Press; 2007.
  2. Twine R. Emissions from animal agriculture-16.5% is the new minimum figure. Sustainability. 2021;13:6276. https://doi.org/10.3390/su13116276
  3. National Academies of Sciences, Engineering, and Medicine. Nutrient requirements of beef cattle. 8th rev ed. Washington, DC: The National Academies Press; 2016.
  4. Lee S, Lee SM, Lee J, Kim EJ. Feeding strategies with total mixed ration and concentrate may improve feed intake and carcass quality of Hanwoo steers. J Anim Sci Technol. 2021;63:1086-97. https://doi.org/10.5187/jast.2021.e88
  5. Liu YF, Sun FF, Wan FC, Zhao HB, Liu XM, You W, et al. Effects of three feeding systems on production performance, rumen fermentation and rumen digesta particle structure of beef cattle. Asian-Australas J Anim Sci. 2016;29:659-65. https://doi.org/10.5713/ajas.15.0445
  6. Moya D, Mazzenga A, Holtshausen L, Cozzi G, Gonzalez LA, Calsamiglia S, et al. Feeding behavior and ruminal acidosis in beef cattle offered a total mixed ration or dietary components separately. J Anim Sci. 2011;89:520-30. https://doi.org/10.2527/jas.2010-3045
  7. Bharanidharan R, Lee CH, Thirugnanasambantham K, Ibidhi R, Woo YW, Lee HG, et al. Feeding systems and host breeds influence ruminal fermentation, methane production, microbial diversity and metagenomic gene abundance. Front Microbiol. 2021;12:701081. https://doi.org/10.3389/fmicb.2021.701081
  8. Statistics Korea. Livestock production survey [Internet]. 2021. [cited 2023 May 9] https://kosis.kr/statHtml/statHtml.do?orgId=101&tblId=DT_1EE0111&conn_path=I2
  9. Bharanidharan R, Arokiyaraj S, Kim EB, Lee CH, Woo YW, Na Y, et al. Ruminal methane emissions, metabolic, and microbial profile of Holstein steers fed forage and concentrate, separately or as a total mixed ration. PLOS ONE. 2018;13:e0202446. https://doi.org/10.1371/journal.pone.0202446
  10. Rajaraman B, Woo YW, Lee CH, Na Y, Kim DH, Kim KH. Effect of feeding method on methane production per dry matter intake in Holstein steers. J Korean Soc Grassl Forage Sci. 2018;38:260-5. https://doi.org/10.5333/KGFS.2018.38.4.260
  11. Holter JB, Urban WE Jr, Hayes HH, Davis HA. Utilization of diet components fed blended or separately to lactating cows. J Dairy Sci. 1977;60:1288-93. https://doi.org/10.3168/jds.S0022-0302(77)84024-1
  12. Lee Y, Bharanidharana R, Park JH, Jang SS, Yeo JM, Kim WY, et al. Comparison of methane production of Holstein steers fed forage and concentrates separately or as a TMR. J Korean Soc Grassl Forage Sci. 2016;36:104-8. https://doi.org/10.5333/KGFS.2016.36.2.104
  13. Kim M, Park T, Yu Z. Metagenomic investigation of gastrointestinal microbiome in cattle. Asian-Australas J Anim Sci. 2017;30:1515-28. https://doi.org/10.5713/ajas.17.0544
  14. Noel SJ, Olijhoek DW, Mclean F, Lovendahl P, Lund P, Hojberg O. Rumen and fecal microbial community structure of Holstein and Jersey dairy cows as affected by breed, diet, and residual feed intake. Animals. 2019;9:498. https://doi.org/10.3390/ani9080498
  15. Kim M. Assessment of the gastrointestinal microbiota using 16S ribosomal RNA gene amplicon sequencing in ruminant nutrition. Anim Biosci. 2023;36:364-73. https://doi.org/10.5713/ab.22.0382
  16. AOAC [Association of Official Analytical Chemists] International. Official methods of analysis of AOAC International. 18th ed. Gaitherburg, MD: AOAC International; 2005.
  17. AOAC [Association of Official Analytical Chemists] International. Official methods of analysis of AOAC International. 18th ed. Gaitherburg, MD: AOAC International; 2006.
  18. Van Soest PJ, Robertson JB, Lewis BA. Methods for dietary fiber, neutral detergent fiber, and nonstarch polysaccharides in relation to animal nutrition. J Dairy Sci. 1991;74:3583-97. https://doi.org/10.3168/jds.S0022-0302(91)78551-2
  19. AOAC [Association of Official Analytical Chemists]. Official methods of analysis. 15th ed. Gaitherburg, MD: AOAC International; 1990.
  20. Song J, Choi H, Jeong JY, Lee S, Lee HJ, Baek Y, et al. Effects of sampling techniques and sites on rumen microbiome and fermentation parameters in Hanwoo steers. J Microbiol Biotechnol. 2018;28:1700-5. https://doi.org/10.4014/jmb.1803.03002
  21. Paz HA, Anderson CL, Muller MJ, Kononoff PJ, Fernando SC. Rumen bacterial community composition in Holstein and Jersey cows is different under same dietary condition and is not affected by sampling method. Front Microbiol. 2016;7:1206. https://doi.org/10.3389/fmicb.2016.01206
  22. Steiner S, Neidl A, Linhart N, Tichy A, Gasteiner J, Gallob K, et al. Randomised prospective study compares efficacy of five different stomach tubes for rumen fluid sampling in dairy cows. Vet Rec. 2015;176:50. https://doi.org/10.1136/vr.102399
  23. Erwin ES, Marco GJ, Emery EM. Volatile fatty acid analyses of blood and rumen fluid by gas chromatography. J Dairy Sci. 1961;44:1768-71. https://doi.org/10.3168/jds.S0022-0302(61)89956-6
  24. Chaney AL, Marbach EP. Modified reagents for determination of urea and ammonia. Clin Chem. 1962;8:130-2. https://doi.org/10.1093/clinchem/8.2.130
  25. Yu Z, Morrison M. Improved extraction of PCR-quality community DNA from digesta and fecal samples. Biotechniques. 2004;36:808-12. https://doi.org/10.2144/04365ST04
  26. Herlemann DPR, Labrenz M, Jurgens K, Bertilsson S, Waniek JJ, Andersson AF. Transitions in bacterial communities along the 2000 km salinity gradient of the Baltic Sea. ISME J. 2011;5:1571-9. https://doi.org/10.1038/ismej.2011.41
  27. Kittelmann S, Seedorf H, Walters WA, Clemente JC, Knight R, Gordon JI, et al. Simultaneous amplicon sequencing to explore co-occurrence patterns of bacterial, archaeal and eukaryotic microorganisms in rumen microbial communities. PLOS ONE. 2013;8:e47879. https://doi.org/10.1371/journal.pone.0047879
  28. Bolyen E, Rideout JR, Dillon MR, Bokulich NA, Abnet CC, Al-Ghalith GA, et al. Reproducible, interactive, scalable and extensible microbiome data science using QIIME 2. Nat Biotechnol. 2019;37:852-7. https://doi.org/10.1038/s41587-019-0209-9
  29. Hall M, Beiko RG. 16S rRNA gene analysis with QIIME2. In: Beiko R, Hsiao W, Parkinson J, editors. Microbiome analysis: methods and protocols. New York, NY: Humana Press; 2018. p. 113-29.
  30. Callahan BJ, McMurdie PJ, Rosen MJ, Han AW, Johnson AJA, Holmes SP. DADA2: high-resolution sample inference from Illumina amplicon data. Nat Methods. 2016;13:581-3. https://doi.org/10.1038/nmeth.3869
  31. Seedorf H, Kittelmann S, Henderson G, Janssen PH. RIM-DB: a taxonomic framework for community structure analysis of methanogenic archaea from the rumen and other intestinal environments. PeerJ. 2014;2:e494. https://doi.org/10.7717/peerj.494
  32. McMurdie PJ, Holmes S. phyloseq: an R package for reproducible interactive analysis and graphics of microbiome census data. PLOS ONE. 2013;8:e61217. https://doi.org/10.1371/journal.pone.0061217
  33. Oksanen J, Blanchet FG, Kindt R, Legendre P, Minchin PR, O'hara R, et al. Package 'vegan'. Community ecology package. Version. 2013;2:1-295.
  34. Andersen KS, Kirkegaard RH, Karst SM, Albertsen M. ampvis2: an R package to analyse and visualise 16S rRNA amplicon data. bioRxiv. 299537 [Preprint]. 2018 [cited 2023 May 9]. https://doi.org/10.1101/299537
  35. Love MI, Huber W, Anders S. Moderated estimation of fold change and dispersion for RNA-seq data with DESeq2. Genome Biol. 2014;15:550. https://doi.org/10.1186/s13059-014-0550-8
  36. Wickham H. ggplot2: elegant graphics for data analysis. SpringerCham; 2016.
  37. Kim M, Morrison M, Yu Z. Status of the phylogenetic diversity census of ruminal microbiomes. FEMS Microbiol Ecol. 2011;76:49-63. https://doi.org/10.1111/j.1574-6941.2010.01029.x
  38. Kim KH, Kim KS, Lee SC, Oh YG, Chung CS, Kim KJ. Effects of total mixed rations on ruminal characteristics, digestibility and beef production of Hanwoo steers. J Anim Sci Technol. 2003;45:387-96. https://doi.org/10.5187/JAST.2003.45.3.387
  39. Li DY, Lee SS, Choi NJ, Lee SY, Sung HG, Ko JY, et al. Effects of feeding system on rumen fermentation parameters and nutrient digestibility in Holstein steers. Asian-Australas J Anim Sci. 2003;16:1482-6. https://doi.org/10.5713/ajas.2003.1482
  40. Jonker A, Muetzel S, Molano G, Pacheco D. Effect of fresh pasture forage quality, feeding level and supplementation on methane emissions from growing beef cattle. Anim Prod Sci. 2016;56:1714-21. https://doi.org/10.1071/AN15022
  41. Maulfair DD, Fustini M, Heinrichs AJ. Effect of varying total mixed ration particle size on rumen digesta and fecal particle size and digestibility in lactating dairy cows. J Dairy Sci. 2011;94:3527-36. https://doi.org/10.3168/jds.2010-3718
  42. Pinares-Patino CS, Baumont R, Martin C. Methane emissions by Charolais cows grazing a monospecific pasture of timothy at four stages of maturity. Can J Anim Sci. 2003;83:769-77. https://doi.org/10.4141/A03-034
  43. Bekele AZ, Koike S, Kobayashi Y. Genetic diversity and diet specificity of ruminal Prevotella revealed by 16S rRNA gene-based analysis. FEMS Microbiol Lett. 2010;305:49-57. https://doi.org/10.1111/j.1574-6968.2010.01911.x
  44. Kononoff PJ, Heinrichs AJ. The effect of reducing alfalfa haylage particle size on cows in early lactation. J Dairy Sci. 2003;86:1445-57. https://doi.org/10.3168/jds.S0022-0302(03)73728-X
  45. Le Liboux S, Peyraud JL. Effect of forage particle size and feeding frequency on fermentation patterns and sites and extent of digestion in dairy cows fed mixed diets. Anim Feed Sci Technol. 1999;76:297-319. https://doi.org/10.1016/S0377-8401(98)00220-X
  46. Woodford ST, Murphy MR. Effect of forage physical form on chewing activity, dry matter intake, and rumen function of dairy cows in early lactation. J Dairy Sci. 1988;71:674-86. https://doi.org/10.3168/jds.S0022-0302(88)79606-X
  47. Lana RP, Russell JB, Van Amburgh ME. The role of pH in regulating ruminal methane and ammonia production. J Anim Sci. 1998;76:2190-6. https://doi.org/10.2527/1998.7682190x
  48. Van Kessel JAS, Russell JB. The effect of pH on ruminal methanogenesis. FEMS Microbiol Ecol. 1996;20:205-10. https://doi.org/10.1111/j.1574-6941.1996.tb00319.x
  49. Hunerberg M, McGinn SM, Beauchemin KA, Entz T, Okine EK, Harstad OM, et al. Impact of ruminal pH on enteric methane emissions. J Anim Sci. 2015;93:1760-6. https://doi.org/10.2527/jas.2014-8469
  50. Hook SE, Wright ADG, McBride BW. Methanogens: methane producers of the rumen and mitigation strategies. Archaea. 2010;2010:945785. https://doi.org/10.1155/2010/945785
  51. Liu H, Xu T, Xu S, Ma L, Han X, Wang X, et al. Effect of dietary concentrate to forage ratio on growth performance, rumen fermentation and bacterial diversity of Tibetan sheep under barn feeding on the Qinghai-Tibetan plateau. PeerJ. 2019;7:e7462. https://doi.org/10.7717/peerj.7462
  52. NIAS [National Institute of Animals Science]. Korean feeding standard for Hanwoo. NIAS: Wanju; 2017.
  53. Chandramoni, Jadhao SB, Tiwari CM, Khan MY. Energy metabolism with particular reference to methane production in Muzaffarnagari sheep fed rations varying in roughage to concentrate ratio. Anim Feed Sci Technol. 2000;83:287-300. https://doi.org/10.1016/S0377-8401(99)00132-7
  54. Russell JB, O'Connor JD, Fox DG, Van Soest PJ, Sniffen CJ. A net carbohydrate and protein system for evaluating cattle diets: I. ruminal fermentation. J Anim Sci. 1992;70:3551-61. https://doi.org/10.2527/1992.70113551x
  55. GIR [Greenhouse Gas Information]. National greenhouse gas inventory report of Korea. Seoul: Greenhouse Gas Inventory & Research Center of Korea; 2020.
  56. Jo N, Kim J, Seo S. Comparison of models for estimating methane emission factor for enteric fermentation of growing-finishing Hanwoo steers. SpringerPlus. 2016;5:1212. https://doi.org/10.1186/s40064-016-2889-7
  57. Yurtseven S, Ozturk I. Influence of two sources of cereals (corn or barley), in free choice feeding on diet selection, milk production indices and gaseous products (CH4 and CO2) in lactating sheep. Asian J Anim Vet Adv. 2009;4:76-85. https://doi.org/10.3923/ajava.2009.76.85
  58. Mi L, Yang B, Hu X, Luo Y, Liu J, Yu Z, et al. Comparative analysis of the microbiota between sheep rumen and rabbit cecum provides new insight into their differential methane production. Front Microbiol. 2018;9:575. https://doi.org/10.3389/fmicb.2018.00575
  59. Huang C, Ge F, Yao X, Guo X, Bao P, Ma X, et al. Microbiome and metabolomics reveal the effects of different feeding systems on the growth and ruminal development of yaks. Front Microbiol. 2021;12:682989. https://doi.org/10.3389/fmicb.2021.682989
  60. Asma Z, Sylvie C, Laurent C, Jerome M, Christophe K, Olivier B, et al. Microbial ecology of the rumen evaluated by 454 GS FLX pyrosequencing is affected by starch and oil supplementation of diets. FEMS Microbiol Ecol. 2013;83:504-14. https://doi.org/10.1111/1574-6941.12011
  61. Kamke J, Kittelmann S, Soni P, Li Y, Tavendale M, Ganesh S, et al. Rumen metagenome and metatranscriptome analyses of low methane yield sheep reveals a Sharpea-enriched microbiome characterised by lactic acid formation and utilisation. Microbiome. 2016;4:56. https://doi.org/10.1186/s40168-016-0201-2
  62. Bryant MP, Robinson IM. Some nutritional characteristics of predominant culturable ruminal bacteria. J Bacteriol. 1962;84:605-14. https://doi.org/10.1128/jb.84.4.605-614.1962
  63. Bryant MP. Bacterial species of the rumen. Bacteriol Rev. 1959;23:125-53. https://doi.org/10.1128/br.23.3.125-153.1959
  64. Williams AG, Withers SE, Coleman GS. Glycoside hydrolases of rumen bacteria and protozoa. Curr Microbiol. 1984;10:287-93. https://doi.org/10.1007/BF01577143
  65. Shinkai T, Enishi O, Mitsumori M, Higuchi K, Kobayashi Y, Takenaka A, et al. Mitigation of methane production from cattle by feeding cashew nut shell liquid. J Dairy Sci. 2012;95:5308-16. https://doi.org/10.3168/jds.2012-5554
  66. Watanabe Y, Suzuki R, Koike S, Nagashima K, Mochizuki M, Forster RJ, et al. In vitro evaluation of cashew nut shell liquid as a methane-inhibiting and propionate-enhancing agent for ruminants. J Dairy Sci. 2010;93:5258-67. https://doi.org/10.3168/jds.2009-2754
  67. Danielsson R, Dicksved J, Sun L, Gonda H, Muller B, Schnurer A, et al. Methane production in dairy cows correlates with rumen methanogenic and bacterial community structure. Front Microbiol. 2017;8:226. https://doi.org/10.3389/fmicb.2017.00226
  68. Granja-Salcedo YT, Fernandes RM, de Araujo RC, Kishi LT, Berchielli TT, de Resende FD, et al. Long-term encapsulated nitrate supplementation modulates rumen microbial diversity and rumen fermentation to reduce methane emission in grazing steers. Front Microbiol. 2019;10:614. https://doi.org/10.3389/fmicb.2019.00614
  69. Cotta MA. Interaction of ruminal bacteria in the production and utilization of maltooligosaccharides from starch. Appl Environ Microbiol. 1992;58:48-54. https://doi.org/10.1128/aem.58.1.48-54.1992
  70. Deusch S, Camarinha-Silva A, Conrad J, Beifuss U, Rodehutscord M, Seifert J. A structural and functional elucidation of the rumen microbiome influenced by various diets and microenvironments. Front Microbiol. 2017;8:1605. https://doi.org/10.3389/fmicb.2017.01605
  71. Flint HJ. The rumen microbial ecosystem-some recent developments. Trends Microbiol. 1997;5:483-8. https://doi.org/10.1016/S0966-842X(97)01159-1
  72. Aguilar-Marin SB, Betancur-Murillo CL, Isaza GA, Mesa H, Jovel J. Lower methane emissions were associated with higher abundance of ruminal Prevotella in a cohort of Colombian buffalos. BMC Microbiol. 2020;20:364. https://doi.org/10.1186/s12866-020-02037-6
  73. Carberry CA, Kenny DA, Han S, McCabe MS, Waters SM. Effect of phenotypic residual feed intake and dietary forage content on the rumen microbial community of beef cattle. Appl Environ Microbiol. 2012;78:4949-58. https://doi.org/10.1128/AEM.07759-11
  74. Chen H, Wang C, Huasai S, Chen A. Effects of dietary forage to concentrate ratio on nutrient digestibility, ruminal fermentation and rumen bacterial composition in Angus cows. Sci Rep. 2021;11:17023. https://doi.org/10.1038/s41598-021-96580-5
  75. Liu K, Wang L, Yan T, Wang Z, Xue B, Peng Q. Relationship between the structure and composition of rumen microorganisms and the digestibility of neutral detergent fibre in goats. Asian-Australas J Anim Sci. 2019;32:82-91. https://doi.org/10.5713/ajas.18.0043
  76. McGilliard ML, Swisher JM, James RE. Grouping lactating cows by nutritional requirements for feeding. J Dairy Sci. 1983;66:1084-93. https://doi.org/10.3168/jds.S0022-0302(83)81905-5
  77. Nocek JE, Steele RL, Braund DG. Effect of mixed ration nutrient density on milk of cows transferred from high production group. J Dairy Sci. 1985;68:133-9. https://doi.org/10.3168/jds.S0022-0302(85)80806-7
  78. Janssen PH, Kirs M. Structure of the archaeal community of the rumen. Appl Environ Microbiol. 2008;74:3619-25. https://doi.org/10.1128/AEM.02812-07
  79. Pinares C, Waghorn G. Technical manual on respiration chamber designs [Internet]. 2014 [cited 2022 Sep 9]. https://www.globalresearchalliance.org/wp-content/uploads/2012/03/GRA-MAN-Facility-BestPract-2012-FINAL.pdf