Piper Oil Decreases In Vitro Methane
Production with Shifting Ruminal Fermentation in a Variety of Diets
Rayudika Aprilia Patindra Purba1*,
Chalermpon Yuangklang2, Siwaporn Paengkoum3 and Pramote
Paengkoum1*
1School of Animal Technology and Innovation, Institute
of Agricultural Technology, Suranaree University of Technology, Nakhon
Ratchasima 30000, Thailand
2Department
of Agricultural Technology and Environment, Faculty of Sciences and Liberal
Arts, Rajamangala University of Technology Isan, Nakhon Ratchasima 30000,
Thailand
3Program in Agriculture, Faculty of Science and
Technology, Nakhon Ratchasima Rajabhat University, Nakhon Ratchasima 30000,
Thailand
*For
correspondence: rayudikaapp.007@gmail.com; pramote@sut.ac.th
Received 12 June
2020; Accepted 26 September 2020; Published 10 December 2020
Abstract
The objective of this study was
to investigate the effect of piper oil (PO), alone or in combination with
sunflower oil (SFO), on biogas production, fermentation end-products and
microorganism in the rumen of lactating goats using in vitro
fermentation technique. Basal substrate consisted of pangola hay and
concentrate (50:50), which was modified with the experimental treatments. The
treatments were organized as a completely randomized 3 × 5 factorial arrangement,
whereby 0 (no), 15 (low) and 30 mg (high) SFO were combined with 0, 15, 30, 45
and 60 mg PO on a dry matter basis. Generally, gas accumulation was not affected by supplementation
with SFO treated with 0–30 mg PO. However, provision of exceedingly high PO
dose at 60 mg decreased gas accumulation. These PO influences were a consistent
picture at CO2 yield, system digestibility and total volatile fatty
acid (VFA). Noteworthy, an inclusion of 45 mg PO did not affect total VFA in
presence of no, low and high SFO. A significant reduction in CH4
production was observed when 45–60 mg PO was combined with no SFO (up to 32.1%), low SFO (up to 33.3%) and (up
to 33.9%) compared to respective controls. Rumen protozoa were seen to
gradually decrease in the presence of SFO and PO. Total bacterial and fungal
zoospores varied in numbers following different PO supplementations. SFO and PO
supplementations did not change pH, but lowered ammonia levels compared to respective controls. The results of the present
study demonstrate that PO (especially at an inclusion of 45 mg) is as effective
as other methane mitigation agents such as SFO, in reducing emissions, without
negatively impacting rumen fermentation. © 2021 Friends
Science Publishers
Keyword: Biogas; Dairy goat; Eugenol; Environmental
pollution; Rumen
Introduction
Domestic ruminants are the one of the major
contributors to the release of greenhouse gases, so there is mounting interest in reducing such
emissions. Enteric fermentation in ruminants contributes to about 18% of CH4
and 9% of CO2 global emissions (FAO 2006) and consumes 2–12% of
total gross energy intake by these animals (Johnson and Johnson 1995). These
values make ruminants highly inefficient and environmentally unfriendly.
Vegetable oil, microalgae, organic acids, yeast, and tannin-saponin have been
widely used to reduce gas emissions by ruminants (Polyorach et al. 2014; Elghandour et
al. 2017; Naumann et al. 2017).
While reducing enteric CH4 emission, dietary
supplementation with vegetable oil such as sunflower oil (SFO) provides
documented benefits by improving the lifespan-extending bacterial, especially
cellulolytic bacteria (Gao et al.
2016). SFO richer in unsaturated fatty acid content inhibits the growth of
ruminal ciliate protozoa and interfere engulf activity of bacteria by ruminal
protozoa. Dietary SFO, thus, increases total rumen biomass and eventually
surpasses rumen fermentation (Gao et al.
2016). This activity of oil inclusion in both reducing CH4 production and providing additional
nutrients, therefore, has been suggested as a cost-effective (Beauchemin and
McGinn 2006).
Recent strategy by dietary essential oils have shown
potential to decrease CH4 emissions and can alter rumen properties; however,
there are self-imposed restrictions such as inconsistency, impermanent and
adverse effects in their application as feed additives for ruminants (Newbold and Ramos-Morales 2020). Hence, essential
oils that are selected should have a positive impact, at least on fermentation end-products (Benchaar et al. 2008). One such essential oil
component is eugenol (Castillejos et al.
2008); however, its effect takes time to be detected and its efficiency depends
on primary substrate, dose and incubation (Castillejos et al. 2006). Piper oil (PO) is refined essential oil
extracted and isolated from Piper betle L. leaves using water-steam
distillations and PO may have a direct affection on enteric CH4 emission and ruminal fermentation
shift. Eugenol was detected in essential oil of all of the P.
betle L. varieties at the highest concentration value
followed by caryophyllene, safrole and chavicol (Karak et al. 2018; Islam et al.
2020).
Although dietary vegetable oil and essential oil
seem to alleviate enteric CH4
emission and to achieve the environmentally
friendly activities, optimization of their use as a methane inhibitor in
ruminant diets is necessary to be investigated, alone and combination (Newbold
and Ramos-Morales 2020). For instance, essential
oils were added at high dose and this supplementation had deleterious effects
on efficiency of rumen fermentation, palatability and possibly cause toxicity (Benchaar
and Greathead 2011). Nevertheless, negative effects can be evaded at a lower
dose, but the methane mitigation would be dwindled as well (Patra and Yu 2015).
A combination of a low amount of methane inhibitors, either using SFO or
organic compound of P. betle L. leaves, has been reported to reduce
enteric methane production and had only a small influence on feed degradation (Purba et al. 2020b, c). At present, however,
it is not known whether supplementation with PO and SFO has a synergistic
effect and can improve animal performance. We postulated that PO could shift
the ruminal fermentation pathway. Therefore, the objective of this study was to
investigate the effect of PO at five different doses, combined or not with SFO,
on biogas release, fermentation end-products, and microbial composition in
rumen fluids from lactating goats, as estimated by in vitro techniques.
Materials and Methods
All
experimental procedures were approved and carried out in accordance with the
Rules of Animal Welfare and all research on animals was conducted according to
the Institutional Committee on Animal Use (SUT 4/2558).
Substrate, piper oil and treatment
A
standard total mixed ration (TMR) commonly fed to ruminant livestock in
Thailand consisted of pangola hay (Digitaria eriantha) and concentrate
(50: 50) was dedicated as basal substrate (Table 1). To obtain piper oil (PO), P.
betle L. leaves were bought from the local market in Prachinburi in eastern
Thailand, collected, dusted and placed into a Clevenger apparatus together with
deionized water at a 1:4 ratio and incubated for 2 h. Steam distillation
products were rinsed, separated and collected using hexane. Hexane was
completely removed using a Rotavapor (R-300; Büchi, Switzerland). To quantify the content
of eugenol, 20 µL
PO was injected into a 1260 Infinity instrument
Table 1: Ingredients and chemical composition of basal diet (g/kg DM, otherwise
stated)
Item |
Basal diet |
Ingredients |
|
Pangola Hay |
500 |
Cassava chip |
30 |
Cassava pulp |
192 |
Mineral1 |
8 |
Molasses |
40 |
Palm meal |
130 |
Premix1 |
2 |
Rice bran |
48 |
Soybean meal |
40 |
Sulfur |
1 |
Urea |
9 |
Chemical composition |
|
Organic matter |
941 |
Crude protein |
108 |
Ether extract |
24 |
Neutral detergent fibre |
685 |
Acid detergent fibre |
595 |
Fatty acid (FA) composition
(in g/100 g FA) |
|
C16:0 |
5.12 |
C18:0 |
0.26 |
C18:2n-6 |
4.95 |
C18:3n-3 |
0.07 |
1Mineral and premix uses a similar
commercial product as given by Purba et
al. (2020b).
(Agilent Technologies, USA) for high-performance liquid
chromatography (HPLC) with diode-array detection and mobile phase consisting of
1:9 HPLC-grade acetonitrile: acetic
acid (1%) (Purba and Paengkoum 2019). Separation was achieved by a
reversed-phase Zorbax SB-C18 column (3.5-µm
particle size, i.d. 4.6 mm × 250 mm). A standard stock solution was prepared
using commercial eugenol (Sigma-Aldrich, USA). Data collection was performed using OpenLAB CDS v. 1.8.1 (Agilent
Technologies). All measurements were performed in triplicate and chemical
standards were included in each analytical run as appropriate. Eugenol content
in PO was estimated at 20 g/kg DM.
Treatments followed a 3 × 5
factorial arrangement in a completely randomized design, whereby three doses of
SFO (0, 15 and 30 mg) were combined with five doses of PO (0, 15, 30, 45 and 60
mg) on a dry matter (DM) basis. SFO composition (in g/kg fatty acid) was as
follows: 16:0 (51.07), 18:0 (27.36), cis-9
18:1 (355.43), 18:2n-6 (422.24), and 18:3n-3 (1.74). SFO and PO emulsified in a
1:99 v/v 96% ethanol: aqueous solution, then decanted into a glass syringe. The
glass syringes that contained 0 mg of PO in presence of three doses of SFO (0,
15, and 30 mg) were designated as the respective control treatment. Selected
doses of SFO and PO in present study were based on the summary of prior studies
(Calsamiglia et al. 2007; Elghandour et al. 2017; Purba et al. 2020a, b).
In vitro incubation
Rumen fluids were collected from four
lactating Saanen goats (body weight, 41 ± 1.37 kg) via oral lavage using a suction pump (CV-SF18; Hitachi, Japan)
before morning feeding time (Tian et al.
2018) and following a 15-day adaptation period on the TMR (basal substrate).
All preparation and in vitro gas production measurements were performed
according to the protocol by Menke and Steingass (1988), as modified by Paengkoum
(2019), and were conducted in Nakhon Ratchasima, Thailand (14°52’36’’N,
102°00’54’’E; elevation above 200 m). Briefly, collected rumen fluid was kept
in a pre-warmed thermal flask, then strained using a nylon membrane (400 µm;
Fisher Scientific S.L., Madrid, Spain) into a conical flask, and mixed with
salivary buffer (1:2, mL: mL) under CO2 and kept at 39°C. The
composition of the rumen fluid buffer mixture was as follows: 474 mL rumen
fluid, 0.60 g MgSO4.7H2O, 1.32 g CaCl2.2H2O,
0.10 g MnCl2.4H2O, 0.10 g CoCl2.6H2O,
0.80 g FeCl3.6H2O, 35 g NaHCO3, 4 g NH4HCO3,
5.70 g Na2HPO4, 6.20 g KH2PO4, 10
mg resazurin and 0.40 g NaOH, made up to 1000 mL with distilled water (Menke
and Steingass 1988). Each hundred Hohenheim glass syringes containing the prior
SFO and PO treatment combinations were added to 500 mg of basal substrate. For
example, the control treatment contained 500 mg of basal substrate, 0 mg of SFO
and 0 mg of PO. The glass syringes were then added 30 mL of rumen fluid buffer
mixture as a final preparation prior to incubation. Once the glass syringes
were locked with three-way stopcocks and capped by glass plungers, the glass
syringes were subsequently shaken and placed in a water bath set at 39°C. The
incubation was run for 72 h, with shaking once per hour. All incubations were
completed in ten replications and three runs on separate days, and gas
production was corrected for every run with three blanks containing rumen
mixture only. Gas production was read after 0, 2, 4, 6, 8, 10, 12, 24, 36, 48
and 72 h. To calculate the cumulative volume of gas production, the measured
value was fitted to the model of Orskov and Mcdonald (1970):
y = a
+ b [1-e(−ct)]
Where a (mL/g DM) is gas production from the
soluble fraction, b is gas production from the insoluble fraction (mL/g DM), c
(/h) is the gas production rate constant for the insoluble fraction (b), t (h)
is the incubation time, (a + b) (mL/g DM) is the potential gas production, and
y is the gas produced at time ‘t’ (mL/g DM).
Laboratory analysis and sampling
DM was
prepared (#950.02; AOAC) and analyzed (#925.04; AOAC) from 2.0 g of ground
sample after drying in a forced-air oven at 105°C for 4 h (AOAC 2005). Organic
matter content was calculated as OM = 100% - ash %; the latter was obtained
after incineration in a muffle furnace at 550°C for 5 h (#942.05; AOAC) (AOAC
2005). Total N was measured using the Kjeldahl method and crude protein
concentration was calculated as total N × 6.25 (#984.13; AOAC) (AOAC 2005).
Ether extract concentration was measured by extraction with petroleum ether
(#920.39; AOAC) (AOAC 2005) and fatty acid concentration was calculated from
methylation using a gas chromatographer (7890A; Agilent Technologies, USA), with external standards
(Supelco 37-Component FAME Mix; Supelco Inc., USA) (Weirdt et al. 2013).
Concentrations of acid-detergent fiber and neutral-detergent fiber were
measured by sequential analysis without amylase (substituted by sodium sulfite)
and were expressed by excluding residual ash ( Soest et al. 1991). Gross energy was determined using a Parr 6200 bomb
calorimeter with O2 as carrier gas (Parr Instruments Co., USA) according to the manufacturer’s instructions.
All measurements were performed in triplicate and chemical standards were
included in each analytical run as appropriate.
Gas production at 0, 2, 4,
6, 8, 10, 12, 24, 36, 48, and 72 h was directly read using a pressure
transducer and a calibrated syringe as specified by Theodorou et al. (1994). Each run of the in
vitro incubation contained 10 replicated glass syringes. Five replicated
glass syringes were used for sample analysis at 24 h and five glass syringes
were used for sample analysis after 72 h of incubation. At 24 and 72 h, 10 mL
of the gas collected from two glass syringes was dispatched into the gas
chromatographer to measure CH4 and CO2 levels (mL/g DM).
When glass syringes were unplugged, the pH was immediately measured using a pH
meter (pH 700; Oakton, USA). The rumen fluid was filtered
and rumen content was collected through pre-weighed Gooch crucibles and
residual DM was estimated. The percent loss in weight was calculated and in
vitro DM degradability (IVDMD) was derived. The dried feed sample and
remaining residue from above were incinerated in a furnace at 550°C for 5 h to
determine in vitro OM degradability. Finally, IVDMD samples were
observed following the neutral-detergent fiber protocol (Frutos et al. 2004) to measure in vitro true
substrate digestibility.
After 24 h, rumen fluids of remaining glass syringes
were filtered through four layers of cheesecloth. Once the glass syringes were
unplugged, pH was immediately measured using a pH meter as above. Samples were
divided into two aliquots. The first aliquot was centrifuged at 6,000 × g at
4°C for 15 min, and the supernatant was stored at -20°C before NH3-N
analysis using the micro-Kjeldahl method (8100; Foss Kjeltech, USA) (AOAC 2005)
and volatile fatty acids (VFA) detection by gas chromatography (HP 6890;
Hewlett Packard, USA) (Erwin et al.
1961). The second aliquot was prepared and fixed with 10% formalin solution in
a sterilized 0.9% saline solution to assess microorganism numbers in a counting
chamber (Neubauer-Boeco, Germany). Specifically, the fixed solution was diluted
100 ×, 10 ×, and 10 × with autoclaved deionized water to count total bacteria,
fungal zoospores, and protozoa using 10 × 40, 10 × 40, and 10 × 10 (ocular ×
objective) magnification, respectively (Galyean 1989). The dilution and
magnification settings for quantifying microbial composition were different due
to varying sizes of bacteria, fungal zoospore and protozoa.
Statistical analysis
Due to
outcomes in consecutively runs was similar (we tested in preliminary
statistical tabulation; not significant different, P < 0.05), data
were averaged and subjected to analysis of variance. All data were analyzed as
a 3×5 factorial arrangement in a completely randomized design using the PROC
GLM of S.A.S. 9.4 software (S.A.S. Institute Inc., 2015, USA). Data were analyzed using the
model:
Yij = µ+Ai + Bj + ABij+ €ij
where: Y = observations; µ = overall mean; Ai = effect
of factor A (SFO supplementation, i = 1 to 3); Bj = effect of factor
B (level of PO, j = 1 to 5), ABij = interaction between factor
A and B, and €ij = the residual effect. Multiple comparisons among
SFO supplementation, PO treatment and combination of SFO and PO were assessed
using Tukey’s honestly significant difference (Kaps
and Lamberson 2004). Differences among means were considered
statistically significant at P < 0.05. The trend of differences in CO2
yield and CH4 production were assessed by orthogonal contrast (P
< 0.05).
Results
Effect
of substrate supplemented with or without sunflower oil (SFO) treated by piper
oil (PO) on gas cumulative, in vitro degradability and in vitro
true substrate digestibility at 24 and 72 h after incubation is presented in
Table 2. In general, gas accumulation was not affected by supplementation with
SFO treated with 0–30 mg PO during 72 h of incubation (Fig. 1). However,
provision of exceedingly PO dose at 45–60 mg decreased gas accumulation (P
< 0.001). Substrate supplemented with or without SFO with 0–30 mg PO
maintained system degradability and digestibility, but those showed a downward
trend (P < 0.05) at 45–60 mg PO in all substrates; In addition,
providing PO produced a consistent picture at different incubated times. No
interaction was found on all parameters in Table 2 (P > 0.05).
The effect of treatments on CO2 is
shown in Fig. 2a and can be summarized by no apparent change in CO2
yield after 24 and 72 h of incubation (P > 0.05). A significant drop
in CO2 was observed only with 45–60 mg PO in all substrates 24 and
72 h of incubation (P < 0.05). As shown in Fig. 2b, a significant
reduction (P < 0.001) in CH4 production was observed at 24
h of incubation with 45–60 mg PO in the presence of no SFO (up to 36.0%), low
SFO (up to 38.3%) and (up to 39.8%) compared to respective controls;
Furthermore, a significant reduction (P < 0.001) in CH4
production was obtained in similar numbers at terminated incubation with 45–60
mg PO in all substrates (up to 28.0% in all cases) compared to respective
controls. Collectively,
PO alleviated CH4 production during substrate 72 h of incubation that was at no SFO (up to 32.1%), low SFO (up to 33.3%) and (up
to 33.9%)
Fig. 1: The cumulative gas production
trend of substrates supplemented with or without sunflower oil (SFO) treated
piper oil (PO). (a) No SFO, 0 mg; (b) Low SFO, 15 mg; (c) High SFO, 30 mg. Data reported as
least-squares ± a standard error of mean (N=30)
compared to respective controls.
Effect of substrate supplemented with or
without SFO treated by PO on in vitro volatile fatty acid (VFA) is
presented in Table 3. SFO increased total VFA (P = 0.001). Total VFA
remained unchanged after 0–30 mg PO added in substrate (P > 0.05).
However, a significant decrease in total VFA was observed only with 45–60 mg PO
in all substrates supplemented with no, low and high SFO (P < 0.001).
There was interaction between SFO supplementation and PO dose for ratio of
acetate to propionate and propionate fraction as well (P < 0.001). PO
increased acetate (P < 0.001), but the trend was reversed when 45–60
mg PO were added in all substrates. Butyric acid was generally more abundant
compared to each respective control after treated with PO (P < 0.001)
and did not change branched-chain fatty acids (iso fraction of butyric and
valeric acids).
SFO and PO supplementation did not generally
alter the pH (P > 0.05); however, ammonia gradually decreased in
conjunction with SFO and PO (P < 0.05) towards the respective
controls (Table 4). Likewise, composition of the ruminal microbial community
was altered by the presence of SFO and PO. SFO modulated total bacteria (P
= 0.029). While total bacteria remained constant in number after
supplementation with SFO and PO (P > 0.05), their amount dropped
substantially (P = 0.003) after treated with PO at 60 mg per DM (Table
4). There was interaction between SFO supplementation and PO dose for protozoa
and fungal zoospore (P < 0.05). The presence of SFO and PO slightly
Parameter |
Time (h) |
PO (mg) |
Supplementation
of SFO1 |
SEM2 |
Comparison |
||||
No |
Low |
High |
SFO |
PO |
Interaction |
||||
Gas cumulative (mL/g DM) |
24 |
0 |
190.9a |
190.4a |
190.9a |
0.844 |
0.177 |
< 0.001 |
0.077 |
|
|
15 |
190.6a |
190.5a |
190.9a |
|
|
|
|
|
|
30 |
190.0a |
190.6a |
191.1a |
|
|
|
|
|
|
45 |
181.9b |
180.4b |
181.9b |
|
|
|
|
|
|
60 |
174.1c |
175.6c |
180.1c |
|
|
|
|
|
72 |
0 |
202.0a |
201.5a |
199.8a |
0.890 |
0.063 |
< 0.001 |
0.370 |
|
|
15 |
204.0a |
200.5a |
195.5a |
|
|
|
|
|
|
30 |
202.4a |
201.9a |
199.4a |
|
|
|
|
|
|
45 |
191.7b |
190.2b |
189.7b |
|
|
|
|
|
|
60 |
183.3c |
187.8c |
184.8c |
|
|
|
|
In vitro dry matter
degradability (g/100 g DM) |
24 |
0 |
45.4a |
45.5a |
45.4a |
0.205 |
0.719 |
0.010 |
0.997 |
|
|
15 |
45.3a |
45.4a |
45.6a |
|
|
|
|
|
|
30 |
45.3a |
45.5a |
45.5a |
|
|
|
|
|
|
45 |
45.1a |
45.0a |
45.2a |
|
|
|
|
|
|
60 |
44.3b |
44.5b |
44.5b |
|
|
|
|
|
72 |
0 |
48.2a |
48.5a |
48.3a |
0.219 |
0.612 |
0.020 |
0.524 |
|
|
15 |
49.0a |
48.3a |
48.3a |
|
|
|
|
|
|
30 |
48.8a |
48.5a |
48.3a |
|
|
|
|
|
|
45 |
48.1a |
48.2a |
48.2a |
|
|
|
|
|
|
60 |
47.6b |
47.6b |
47.6b |
|
|
|
|
In vitro organic
matter degradability (g/100 g DM) |
24 |
0 |
52.5a |
52.4a |
52.5a |
0.236 |
0.961 |
0.001 |
0.482 |
|
|
15 |
52.3a |
52.8a |
52.6a |
|
|
|
|
|
|
30 |
52.4a |
52.5a |
52.7a |
|
|
|
|
|
|
45 |
51.9b |
51.1b |
51.4b |
|
|
|
|
|
|
60 |
50.2c |
50.1c |
50.3c |
|
|
|
|
|
72 |
0 |
59.5a |
59.1a |
59.4a |
0.267 |
0.738 |
0.002 |
0.818 |
|
|
15 |
59.3a |
59.5a |
59.3a |
|
|
|
|
|
|
30 |
59.1a |
59.3a |
59.2a |
|
|
|
|
|
|
45 |
58.3b |
57.9b |
58.7b |
|
|
|
|
|
|
60 |
57.5c |
57.2c |
57.4c |
|
|
|
|
In vitro true
substrate digestibility (g/100 g DM) |
24 |
0 |
46.4a |
46.5a |
46.6a |
0.209 |
0.161 |
< 0.001 |
0.665 |
|
|
15 |
46.1a |
46.4a |
46.6a |
|
|
|
|
|
|
30 |
45.8a |
46.5a |
46.5a |
|
|
|
|
|
|
45 |
45.6a |
46.0a |
46.4 a |
|
|
|
|
|
|
60 |
44.2b |
44.1b |
44.2b |
|
|
|
|
|
72 |
0 |
50.3a |
50.5a |
50.3a |
0.228 |
0.919 |
0.007 |
0.129 |
|
|
15 |
50.6a |
50.3a |
50.3a |
|
|
|
|
|
|
30 |
50.5a |
50.5a |
50.3a |
|
|
|
|
|
|
45 |
50.3a |
50.2a |
50.2a |
|
|
|
|
|
|
60 |
49.1b |
49.2b |
49.1b |
|
|
|
|
Fig. 2: The carbon
dioxide yield (Fig. 2a) and methane production (Fig. 2b) of substrates treated
by piper oil (PO) after 24 and 72 h incubation, with different superscript
compared to similar time, meaning significantly different (P < 0.05;
Tukey HSD). Differences among main effects of substrates were performed by
Orthogonal contrast (P < 0.05) with P > 0.05 (ns). Data
reported as least-squares ± standard error of mean (N=21)
Parameter |
PO (mg) |
Supplementation of SFO1 |
SEM2 |
Comparison |
||||
No |
Low |
High |
SFO |
PO |
Interaction |
|||
Total VFA (mmol/L) |
0 |
66.6c |
71.9b |
76.7a |
0.324 |
0.001 |
< 0.001 |
0.222 |
|
15 |
66.8c |
72.0b |
76.9a |
|
|
|
|
|
30 |
67.1c |
72.2b |
77.1a |
|
|
|
|
|
45 |
67.1c |
72.1b |
77.0a |
|
|
|
|
|
60 |
63.2d |
66.5c |
72.4b |
|
|
|
|
Acetate (mol/ 100 mol) |
0 |
54.8c |
54.8c |
54.8c |
0.261 |
0.372 |
< 0.001 |
0.318 |
|
15 |
57.5b |
58.4b |
59.7b |
|
|
|
|
|
30 |
58.9a |
59.4a |
59.8a |
|
|
|
|
|
45 |
59.7b |
57.8b |
56.9b |
|
|
|
|
|
60 |
57.3c |
56.1c |
56.0c |
|
|
|
|
Propionate (mol/ 100 mol) |
0 |
20.7Ra |
21.7Qa |
22.8Pa |
0.088 |
0.012 |
< 0.001 |
< 0.001 |
|
15 |
18.7Qc |
18.7Qc |
19.4Pb |
|
|
|
|
|
30 |
18.5Rc |
18.6Qc |
18.8Pc |
|
|
|
|
|
45 |
18.5Rc |
18.5Rc |
18.7Qc |
|
|
|
|
|
60 |
18.4Rc |
18.5Rc |
18.6Qc |
|
|
|
|
Isobutyrate (mol/ 100 mol) |
0 |
4.5 |
4.2 |
4.0 |
0.019 |
0.395 |
0.072 |
0.105 |
|
15 |
4.4 |
4.3 |
4.1 |
|
|
|
|
|
30 |
4.4 |
4.2 |
4.2 |
|
|
|
|
|
45 |
4.1 |
4.1 |
4.1 |
|
|
|
|
|
60 |
4.4 |
4.3 |
4.1 |
|
|
|
|
Butyrate (mol/ 100 mol) |
0 |
11.0c |
10.9c |
10.9c |
0.052 |
0.243 |
< 0.001 |
0.057 |
|
15 |
11.5b |
11.3b |
11.6b |
|
|
|
|
|
30 |
11.5b |
11.6b |
11.7b |
|
|
|
|
|
45 |
11.2b |
11.2b |
11.1b |
|
|
|
|
|
60 |
12.1a |
12.4a |
12.3a |
|
|
|
|
Isovalerate (mol/ 100 mol) |
0 |
3.3 |
3.3 |
3.2 |
0.016 |
0.352 |
0.800 |
0.997 |
|
15 |
3.2 |
3.4 |
3.0 |
|
|
|
|
|
30 |
3.2 |
3.3 |
3.0 |
|
|
|
|
|
45 |
3.1 |
3.3 |
3.2 |
|
|
|
|
|
60 |
3.2 |
3.4 |
3.1 |
|
|
|
|
Valerate (mol/ 100 mol) |
0 |
5.7a |
5.1a |
4.2b |
0.021 |
0.026 |
< 0.001 |
0.071 |
|
15 |
4.7a |
3.9b |
2.2c |
|
|
|
|
|
30 |
3.4c |
2.8c |
2.4c |
|
|
|
|
|
45 |
3.4c |
5.1a |
5.9a |
|
|
|
|
|
60 |
4.6b |
5.3a |
5.8a |
|
|
|
|
Acetate:Propionate |
0 |
2.6Pc |
2.5Qc |
2.4Rc |
0.014 |
0.014 |
< 0.001 |
<0.001 |
|
15 |
3.1Qa |
3.1Qa |
3.1Qa |
|
|
|
|
|
30 |
3.2Pa |
3.2Pa |
3.2Pa |
|
|
|
|
|
45 |
3.2Pa |
3.1Qa |
3.0Ra |
|
|
|
|
|
60 |
3.1Qa |
3.0 Ra |
3.0Ra |
|
|
|
|
Means
followed by different
superscript (a, b, c) differ at P < 0.05 for the PO effect in substrate; with different
superscripts (P, Q, R) at P < 0.05 for the SFO effect in substrate
lowered the number of total protozoa (P =
0.001); whereas fungal zoospores remained at comparable numbers (P >
0.05), except after addition of 45–60 mg PO, whereby they exhibited a slight
increase (P = 0.001).
Discussion
Modulating rumen fermentation by preventing
the release of environmentally damaging biogases derived from domestic
ruminants has attracted more attention in recent years. Strategies in this
direction include supplementing animal feed with SFO (Elghandour et al. 2017; Vargas et al. 2017), dietary tannin-saponin (Naumann et al. 2017; Cherdthong et
al. 2019b) and yeast (Polyorach et
al. 2014). Selected dietary polyphenol compounds, such as flavonoids (e.g.,
quercetin) and essential oils (e.g., eugenol), seem to play a similar
role (Castillejos et al. 2006;
Lourenço et al. 2014; Kim et al. 2015). Flavonoids and essential
oils of piper powder has been recently shown to modulate rumen fermentation by
increasing fermentable organic matter in substrate containing abundance of
vegetable oil (Purba et al. 2020c).
However, the role of a single essential oil component (e.g., eugenol)
ingested through feed on ruminal activity remains to be determined. The present
discussion, thus, highlighted the use of PO combined with or without SFO in a
feeding regimen via in vitro
measurements.
Rumen
perform an aerobic metabolism, which allows their host to derive energy from
nutrient fermentation (Olagaray and Bradford 2019). This same fermentation
process causes the release of ruminal biogases, measured as total production of
Parameter |
PO (mg) |
Supplementation of SFO1 |
SEM2 |
Comparison |
||||
No |
Low |
High |
SFO |
PO |
Interaction |
|||
pH |
0 |
6.9 |
6.8 |
6.8 |
0.021 |
0.901 |
0.937 |
0.967 |
|
15 |
6.8 |
6.8 |
6.8 |
|
|
|
|
|
30 |
6.8 |
6.8 |
6.8 |
|
|
|
|
|
45 |
6.8 |
6.8 |
6.8 |
|
|
|
|
|
60 |
6.8 |
6.8 |
6.8 |
|
|
|
|
Ammonia
(mg/100 mL) |
0 |
17.3a |
17.3a |
17.4a |
0.076 |
0.107 |
0.011 |
0.266 |
|
15 |
17.1b |
16.8b |
16.7b |
|
|
|
|
|
30 |
17.0b |
16.7b |
16.1b |
|
|
|
|
|
45 |
16.9b |
16.6b |
15.7b |
|
|
|
|
|
60 |
16.1b |
16.4b |
15.5b |
|
|
|
|
Ruminal
microbes (cells/mL) |
|
|
|
|
|
|
|
|
Total
bacteria (×107) |
0 |
7.5c |
7.8b |
8.2a |
0.034 |
0.029 |
0.003 |
0.321 |
|
15 |
7.4c |
7.7b |
7.9a |
|
|
|
|
|
30 |
7.3c |
7.7b |
7.8b |
|
|
|
|
|
45 |
7.3c |
7.6b |
7.8b |
|
|
|
|
|
60 |
6.6d |
7.1c |
7.2c |
|
|
|
|
Total
protozoal (×105) |
0 |
5.6Pa |
4.4Qa |
3.7Ra |
0.017 |
0.033 |
0.001 |
0.014 |
|
15 |
4.5Qa |
3.7Ra |
3.5Pb |
|
|
|
|
|
30 |
3.6Pb |
3.3Qb |
3.3Qb |
|
|
|
|
|
45 |
3.4Qb |
3.0Pc |
3.0Pc |
|
|
|
|
|
60 |
3.1Pc |
2.8Qc |
2.9Qc |
|
|
|
|
Total fungal
zoospore (×105) |
0 |
3.2Rb |
3.3Qb |
3.5Pb |
0.015 |
0.002 |
0.001 |
0.010 |
|
15 |
3.2Rb |
3.3Qb |
3.5Pb |
|
|
|
|
|
30 |
3.2Rb |
3.3Qb |
3.5Pb |
|
|
|
|
|
45 |
3.3Qb |
3.3Qb |
3.6Pa |
|
|
|
|
|
60 |
3.4Qa |
3.4Qa |
3.6Pa |
|
|
|
|
Means followed by different superscript (a, b, c)
differ at P
< 0.05 for the PO effect in substrate; with different
superscripts (P, Q, R) at P
< 0.05 for the SFO effect in substrate
CO2,
CH4, and H2. Here, total gas production remained
unchanged irrespective of increased supplementation with SFO and PO, which could
be expected given that these compounds constitute relatively unfermentable
nutrient sources. Makkar et al.
(1995) reported that manipulating rumen fermentation by supplementing
carbohydrate, protein, and fat content in feed substrate resulted in increased
gas production, although fats led generally to lower increases compared to
carbohydrates and proteins. As a result, more readily fermentable nutrient
sources such as carbohydrates were a major contributor to ruminal biogases (Orskov
and Mcdonald 1970). In the present study, the carbohydrate content of feed
substrate was equal at the onset of each treatment (basal substrate; 500
mg/incubation). Therefore, the lack of change in cumulative gas production
resulted solely from inhibition of carbohydrate fermentation by rumen
microorganisms during incubation, as evidenced also by prior studies (Elghandour et al. 2017; Vargas et al. 2017).
In
present study, PO supplementation at abundant dose markedly causes substrate
disappearance to stagnate during incubation. Adding an excess of PO can inhibit
microbial fermentation activity. Castillejos
et al. (2006) confirmed that eugenol played a major role in suppressing
microbial rumen activity in a long-term fermentation study. Cardozo et al. (2006), who tested a combination
of eugenol and cinnamaldehyde, which had a substantially more severe effect on
rumen fermentation, particularly on fermented DM and OM, than eugenol alone.
The reduction in in vitro degradability of DM and OM in the presence of
60 mg PO per DM, as applied also in the present study, was ascribed to the
limited metabolic capacity of rumen microorganisms and, hence, their inability
to undertake nutrient fermentation (Polyorach et al. 2014). Lower fermentation and degradation activities
depleted also the energy supply of the rumen microflora. This pattern was in
line with previous studies (Castillejos et
al. 2006; Lourenço et al. 2014),
whereby fermentation was strongly inhibited in the presence of elevated doses
of eugenol. In present study, large inhibition
of fermentation and degradation activity was in consistent with alleviated
total gas accumulation in presence of exceedingly high PO dose at 60 mg. The
present findings are consistent with earlier in vivo studies reporting
that SFO and eugenol at acceptable doses did not alter
digestibility in any apparent way (Benchaar
et al. 2012; Atikah et al. 2018).
Dietary
supplementation with vegetable oil such as SFO provides documented benefits by
enhancing the sustainable existence of cellulolytic bacteria (Gao et al. 2016). The unsaturated bonding
of free fatty acid restricts the growth of ruminal ciliate protozoa and limits
the engulfing of bacteria by ruminal protozoa. As a consequence, total rumen
biomass augments, favoring fermentation (Gao
et al. 2016). In line with these observations, the present SFO
supplementation led to higher total VFA, confirming an earlier report by Vargas et al. (2017) and an in vivo
study on dietary SFO supplementation in a goat feeding regimen (Atikah et al. 2018).
Here,
the presence of exceedingly high PO dose reversed the fermentation performance.
While abundant PO dose did not alter total VFA and branched-chain fatty acids,
it affected the proportions of acetate and butyrate and reduced those of
propionate and valerate. These findings were expected given the role of eugenol
in mediating feedback from cellulolytic activity involving prominent
fiber-degraders (Vargas et al. 2017).
Here, the amount of fiber fraction was similar among all treatments. As a
result, eugenol derived from PO could alter the proportion of VFA. In a
previous study, eugenol successfully suppressed propionic acid without
affecting acetic and butyric acid (Castillejos et al. 2006); however, Lourenço
et al. (2014) reported that eugenol supplementation decreased propionic
acid, but ensured elevated proportions of acetic, butyric, valeric, and
branched-chain fatty acids. The slow substrate disappearance observed in the
present study may confirm the inhibitory effect of eugenol on propionic
bacteria and particularly on the generation of intermediates by the propionic
acid pathway, eventually leading to lower propionic acid accumulation (Mitsumori
and Sun 2008; Cherdthong et al.
2019b). A possible reason for the difference between previous reports and
present results may be related to eugenol purity. Even if eugenol was
successfully extracted from PO and quantified, it might nevertheless be
contaminated with other volatile compounds, such as caryophyllene (Islam et al. 2020; Purba et al. 2020d). Hence, PO still contained of caryophyllene may have
a direct antimicrobial affection for inhabitant propionic bacteria, but
caryophyllene may reduce efficiency of eugenol itself. In this sense, the
observed shift of fermentation end-products from acetic to propionic acid is
identical to that reported earlier (Busquet
et al. 2006; Lourenço et al.
2014; Joch et al. 2016).
Rumen
fermentation is accompanied by the release of CO2, H2,
and CH4, mostly as a result of hexose hydrolysis (Wolin 1979). In
the present study, PO supplementation forced rumen microorganisms to optimize
energy consumption, favoring the production of CO2. Nevertheless, an
excessive amount of PO led to a decrease in CO2 yield. Chaves et al. (2008) reported previously that
a general mode of action of essential oils was to decrease CO2 volumes
while augmenting the propionic fraction. However, the effect of eugenol itself
on reducing the CO2 volume remains unclear. According to Mitsumori
and Sun (2008), CO2 release is intimately linked to the
VFA-producing pathway and particularly acetate, propionate, and butyrate
yields. Given that cellulose and hexose content remained constant in this
study, the changes in cumulative CO2 likely reflected VFA
production. Mitsumori and Sun (2008) noted also that the increased volume of CO2
linked to pyruvate metabolism was a consequence of abundant pyruvate-producing
bacteria in the rumen, including Ruminococcus flavefaciens, Fibrobacter succinogens, and
Ruminococcus albus. Vargas et al.
(2017) confirmed that SFO supplementation during fermentation maintained in
check the number of F. succinogens and R. albus. Earlier, Cobellis et al. (2016) reported that adding
essential oils increased F. succinogens numbers but had no effect on the
population of R. flavefaciens and R. albus. While the
identification of specific ruminal microorganisms was outside the scope of the
present study, it is possible that eugenol derived from PO interacted with R.
flavefaciens, F. succinogens,
and R. albus to affect overall CO2 yields.
The
presence of SFO and PO could alleviate CH4 production by increasing
the ratio of acetic to propionic acid. The extent of methane mitigation by SFO
and PO was similar compared to that reported by earlier studies (Joch et al. 2016; Elghandour et al. 2017; Vargas et al. 2017). This result suggested that SFO and PO favored acetogenesis
rather than methanogenesis in the rumen. Previous evidence has highlighted that
CH4 formation is a natural outcome of CO2 and H2
consumption during methanogenesis (Mitsumori and Sun 2008) and propionic acid
plays a major role in the uptake of H2 (Ochoa-García et al. 2019). In other words, increased
propionic acid synthesis sequesters H2 away from methanogenesis,
thus lowering CH4 production (Murali et al. 2017). However, a low proportion of propionic acid, as
observed here, may mean that CO2 and H2 are re-routed
towards acetogenesis as in Blautia acetogenic bacteria (Greening et al. 2019), leading to acetic acid
formation via the Wood-Ljungdahl pathway (Ni
et al. 2011).
Other
fermentation end-products such as ammonia were generally lower in the presence
of SFO and PO. This fact could be attributed to the high level of eugenol and
sunflower oil, as supplementary agents could interfere with the deamination
pathway (Cardozo et al. 2006; Atikah et al. 2018). Busquet et al. (2006) reported that higher
ammonia inhibition was a result of increased butyric and decreased
branched-chain fatty acid accumulation. All rumen fermentation performances in
this study, including VFA and ammonia production, appeared independent of pH,
confirming similar results from previous studies (Busquet et al. 2006; Castillejos et
al. 2006; Joch et al. 2016) and
further supporting a role of ruminal microorganisms. The range of pH and
ammonia content in the present study was 6.8–6.9 and 15.5–17.3 mg/100 mL,
respectively, which was appropriate for microorganisms performing fermentation
in the rumen (Ørskov and MacLeod 1982).
The
present study detected a change in the composition of ruminal microorganisms,
including protozoa, total bacteria, and fungal zoospores following SFO and PO
supplementation. The amount of total bacteria remained unchanged following
addition of SFO, supporting a previous report by Vargas et al. (2017), who suggested that SFO was not capable of enhancing
bacterial activity and especially not that of cellulolytic bacteria. Instead,
an elevated amount of PO correlated with a reduction in methanogenic bacteria.
This could explain the observed reduction in CH4 formation, as
methanogens failed to optimize CO2 and H2 consumption.
Essential oils such as eugenol have been reported to broadly affect the outer
membrane of gram-positive bacteria (Calsamiglia et al. 2007). Once this membrane becomes surrounded by essential
oils, bacteria lose chemiosmotic control over ion gradients, electron
mobilization, phosphorylation cascades, protein translocation, and other
enzymatic reactions (Ultee et al.
2002). Recently, addition of SFO and PO has been shown to suppress ruminal
protozoa, most likely by inhibiting their nucleic acid synthesis (Wanapat et al. 2008; Cherdthong et al. 2019a; Patra and Saxena 2009).
Fungal zoospores were expected to increase in numbers following a reduction in
total protozoa caused by SFO and PO supplementation. However, fungal zoospore
numbers remained unchanged contrasting a previous correlation between fungal
zoospore abundance and fewer ruminal protozoa (Newbold et al. 2015). Fungal zoospores are better equipped than protozoa
to cope with plant defenses including secondary compound such as essential oils
(Cherdthong et al. 2019a). In such
instances, fungal zoospores may be the main microorganisms left to ingest the
remaining ruminal substrate during fermentation.
Conclusion
This study demonstrates that eugenol, the main
compound of piper oil derived from the easily and economically cultivated Piper betle plant, could assist in
mitigating methane production and in improving feed additive utilization during
rumen fermentation by adding 45 mg of piper oil supplementation combined in a
variety of diets. Hopefully, utilizing piper oil can be the cheap alternative
feed additive to be used further application in animal feeding. Here, sunflower
oil is used to provide additional nutrients such lipid as energy through oil
inclusion. As a result, solely piper oil use is as effective as other methane
mitigation agents such as sunflower oil, in reducing emissions, without
negatively impacting rumen fermentation. However, the source of essential oil,
type of basal substrate, and incubation time all interact in different ways to
affect the final outcome, meaning that further studies are required to
determine the optimal combination of these and other factors. Additionally,
dietary piper oil supplementation in an animal feeding regimen should be
analyzed further, to verify which amount can effectively modulate rumen
fermentation while ensuring fail-safe methane mitigation.
Acknowledgments
Authors would like to say thanks to all staffs
of the Centre of Scientific and Technological Equipment and Section of Goat and
Sheep SUT farm, Suranaree University of Technology, and Nurrahim Dwi Saputra
for their valuable helps. Authors would like to extend the heartfelt thanks to
the Laboratory of Monogastric Animal Nutrition and Feed Science for use of
research facilities. This research was funded by Suranaree University of
Technology and by Thailand Science Research and Innovation (TSRI).
Author Contributions
Conceived and designed experiments: RAPP, CY,
SP and PP. Performed the experiments: RAPP and PP. Analyzed the data and wrote
the paper: RAPP, CY, SP and PP.
References
AOAC (2005). Official
methods of analysis. AOAC International Suite 500, Gaitherburg, Maryland,
USA
Atikah IN, AR Alimon, H Yaakub, N Abdullah, MF Jahromi,
M Ivan, AA Samsudin (2018). Profiling of rumen fermentation, microbial
population and digestibility in goats fed with dietary oils containing
different fatty acids. BMC Vet Res 14;
Article 344
Beauchemin KA, SM McGinn (2006). Effects of various feed
additives on the methane emissions from beef cattle. Intl Congr Ser 1293:152‒155
Benchaar C, H Greathead (2011). Essential oils and
opportunities to mitigate enteric methane emissions from ruminants. Anim Feed Sci Technol 166–167:338‒355
Benchaar C, A Lettat, F Hassanat, WZ Yang, RJ Forster,
HV Petit, PY Chouinard (2012). Eugenol for dairy cows fed low or high
concentrate diets: Effects on digestion, ruminal fermentation characteristics,
rumen microbial populations and milk fatty acid profile. Anim Feed Sci Technol 178:139‒150
Benchaar C, S Calsamiglia, AV Chaves, GR Fraser, D
Colombatto, TA McAllister, KA Beauchemin (2008). A review of plant-derived
essential oils in ruminant nutrition and production. Anim Feed Sci Technol 145:209‒228
Busquet M, S Calsamiglia, A Ferret, C Kamel (2006).
Plant extracts affect in vitro rumen
microbial fermentation. J Dairy Sci
89:761‒771
Calsamiglia S, M Busquet, PW Cardozo, L Castillejos, A
Ferret (2007). Invited review: Essential oils as modifiers of rumen microbial
fermentation. J Dairy Sci 90:2580‒2595
Cardozo PW, S Calsamiglia, A Ferret, C Kamel (2006).
Effects of alfalfa extract, anise, capsicum, and a mixture of cinnamaldehyde
and eugenol on ruminal fermentation and protein degradation in beef heifers fed
a high-concentrate diet. J Anim Sci
84:2801‒2808
Castillejos L, S Calsamiglia, J Martín-Tereso, HT Wijlen
(2008). In vitro evaluation of
effects of ten essential oils at three doses on ruminal fermentation of high
concentrate feedlot-type diets. Anim Feed
Sci Technol 145:259‒270
Castillejos L, S Calsamiglia, A Ferret (2006). Effect of
essential oil active compounds on rumen microbial fermentation and nutrient
flow in in vitro systems. J Dairy Sci 89:2649‒2658
Chaves AV, ML He, WZ Yang, AN Hristov, TA McAllister, C
Benchaar (2008). Effects of essential oils on proteolytic, deaminative and
methanogenic activities of mixed ruminal bacteria. Can J Anim Sci 88:117‒122
Cherdthong A, B Khonkhaeng, S Foiklang, M Wanapat, N
Gunun, P Gunun, P Chanjula, S Polyorach (2019a). Effects of supplementation of Piper sarmentosum leaf powder on feed
efficiency, rumen ecology and rumen protozoal concentration in thai native beef
cattle. Animals 9; Article 130
Cherdthong A, R Prachumchai, M Wanapat (2019b). In vitro evaluations of pellets
containing Delonix regia seed meal
for ruminants. Trop Anim Health Prod
51:2003‒2010
Cobellis G, Z Yu, C Forte, G Acuti, M Trabalza-Marinucci
(2016). Dietary supplementation of Rosmarinus
officinalis L. leaves in sheep affects the abundance of rumen methanogens
and other microbial populations. J Anim
Sci Biotechnol 7; Article 27
Elghandour MMY, LH Vallejo, AZM Salem, MZM Salem, LM
Camacho, RG Buendía, NE Odongo (2017). Effects of Schizochytrium microalgae and sunflower oil as sources of
unsaturated fatty acids for the sustainable mitigation of ruminal biogases
methane and carbon dioxide. J Clean Prod
168:1389‒1397
Erwin ES,
GJ Marco, EM Emery (1961). Volatile fatty acid analyses of blood and rumen
fluid by gas chromatography. J Dairy Sci
44:1768‒1771
FAO (2006). Livestock's
Long Shadow e Environmental Issues and Options. Food and Agriculture
Organization, Rome, Italy
Frutos P, G Hervás, FJ Giráldez, AR Mantecón (2004). An in vitro study on the ability of
polyethylene glycol to inhibit the effect of quebracho tannins and tannic acid
on rumen fermentation in sheep, goats, cows and deer. Aust J Agric Res 55:1125‒1132
Galyean M (1989). Laboratory Procedure in Animal
Nutrition Research. Department of Animal and Life Science, New Mexico State
University, Las Cruces, USA
Gao J, MZ Wang, YJ Jing, XZ Sun, TY Wu, LF Shi (2016).
Impacts of the unsaturation degree of long-chain fatty acids on the volatile
fatty acid profiles of rumen microbial fermentation in goats in vitro. J Integr Agric 15:2827‒2833
Greening C, R Geier, CJ Wang, LC Woods, SE Morales, MJ
McDonald, R Rushton-Green, XC Morgan, S Koike, SC Leahy, WJ Kelly, I Cann, GT
Attwood, GM Cook, RI Mackie (2019). Diverse hydrogen production and consumption
pathways influence methane production in ruminants. ISME J 13:2617‒2632
Islam MA, KY Ryu, N Khan, OY Song, JY Jeong, JY Son, N
Jamila, KS Kim (2020). Determination of the volatile compounds in five
varieties of Piper betle L. From
bangladesh using simultaneous distillation extraction and gas
chromatography/mass spectrometry (sde-gc/ms). Anal Lett 53:2413‒2430
Joch M, L Cermak, J Hakl, B Hucko, D Duskova, M Marounek
(2016). In vitro screening of
essential oil active compounds for manipulation of rumen fermentation and
methane mitigation. Asian-Aust J Anim Sci
29:952‒959
Johnson KA, DE Johnson (1995). Methane emissions from
cattle. J Anim Sci 73:2483‒2492
Kaps M, WR Lamberson (2004). Biostatistics for Animal
Science. CABI, Oxfordshire, UK
Karak S, J Acharya, S Begum, I Mazumdar, R Kundu, B De
(2018). Essential oil of Piper betle
L. leaves: Chemical composition, anti-acetylcholinesterase,
anti-β-glucuronidase and cytotoxic properties. J Appl Res Med Aroma 10:85‒92
Kim ET, LL Guan, SJ Lee, SM Lee, SS Lee, ID Lee, SK Lee,
SS Lee (2015). Effects of flavonoid-rich plant extracts on in vitro ruminal methanogenesis, microbial populations and
fermentation characteristics. Asian-Aust
J Anim Sci 28:530‒537
Lourenço M, PW Cardozo, S Calsamiglia, V Fievez (2014).
Effects of saponins, quercetin, eugenol, and cinnamaldehyde on fatty acid
biohydrogenation of forage polyunsaturated fatty acids in dual-flow continuous
culture fermenters. J Anim Sci
86:3045‒3053
Makkar HPS, M Blümmel, K Becker (1995). Formation of
complexes between polyvinyl pyrrolidones or polyethylene glycols and tannins,
and their implication in gas production and true digestibility in in vitro techniques. Brit J Nutr 73:897‒913
Menke KH, H Steingass (1988). Estimation of the
energetic feed value obtained from chemical analysis and in vitro gas production using rumen fluid. Anim Res Dev 28:7‒55
Mitsumori M, W Sun (2008). Control of rumen microbial
fermentation for mitigating methane emissions from the rumen. Asian-Aust J Anim Sci 21:144‒154
Murali N, K Srinivas, BK Ahring (2017). Biochemical
production and separation of carboxylic acids for biorefinery applications. Fermentation 2017; Article 22
Naumann HD, LO Tedeschi, WE Zeller, NF Huntley (2017).
The role of condensed tannins in ruminant animal production: advances,
limitations and future directions. Rev
Bras Zootec 46:929‒949
Newbold CJ, E Ramos-Morales (2020). Review: Ruminal
microbiome and microbial metabolome: Effects of diet and ruminant host. Animal 14:s78‒s86
Newbold CJ, GDL Fuente, A Belanche, E Ramos-Morales, NR
McEwan (2015). The role of ciliate protozoa in the rumen. Front Microbiol 6:1313‒1326
Ni BJ, H Liu, YQ Nie, RJ Zeng, GC Du, J Chen, HQ Yu
(2011). Coupling glucose fermentation and homoacetogenesis for elevated acetate
production: Experimental and mathematical approaches. Biotechnol Bioeng 108:345‒353
Ochoa-García PA, MM Arevalos-Sánchez, O Ruiz-Barrera, RC
Anderson, AO Maynez-Pérez, FA Rodríguez-Almeida, A Chávez-Martínez, H
Gutiérrez-Bañuelos, A Corral-Luna (2019). In
vitro reduction of methane production by 3-nitro-1-propionic acid is
dose-dependent. J Anim Sci 97:1317‒1324
Olagaray KE, BJ Bradford (2019). Plant flavonoids to
improve productivity of ruminants – A review. Anim Feed Sci Technol 251:21‒36
Ørskov E, N MacLeod (1982). The determination of the
minimal nitrogen excretion in steers and dairy cows and its physiological and
practical implications. Brit J Nutr
47:625‒636
Orskov ER, I Mcdonald (1970). The estimation of protein
degradability in the rumen from incubation measurements weighted according to
rate of passage. J Agric Sci Camb
92:499‒503
Paengkoum P (2019). Applied
Goat Nutrition. Korat Marketing and Production, Nakhon Ratchasima,
Thailand.
Patra AK, J Saxena (2009). The effect and mode of action
of saponins on the microbial populations and fermentation in the rumen and
ruminant production. Nutr Res Rev
22:204‒219
Patra AK, Z Yu (2015). Effects of adaptation of in vitro rumen culture to garlic oil,
nitrate, and saponin and their combinations on methanogenesis, fermentation,
and abundances and diversity of microbial populations. Front Microbiol 6; Article 1434
Polyorach S, M Wanapat, A Cherdthong (2014). Influence of
yeast fermented cassava chip protein (YEFECAP) and roughage to concentrate
ratio on ruminal fermentation and microorganisms using in vitro gas production technique. Asian-Aust J Anim Sci 27:36‒45
Purba RAP, P Paengkoum (2019). Bioanalytical HPLC method
of Piper betle L. for quantifying
phenolic compound, water-soluble vitamin, and essential oil in five different
solvent extracts. J Appl Pharm Sci 9:033‒039
Purba RAP, P Paengkoum, S Paengkoum (2020a). The links
between supplementary tannin levels and conjugated linoleic acid (CLA)
formation in ruminants: A systematic review and meta-analysis. PLoS One 15; Article e0216187
Purba RAP, S Paengkoum, C Yuangklang, P Paengkoum
(2020b). Flavonoids and their aromatic derivatives in Piper betle powder promote in
vitro methane mitigation in a variety of diets. Cienc Agrotechnol 44:1–11
Purba RAP, C Yuangklang, P Paengkoum (2020c). Enhanced
conjugated linoleic acid and biogas production after ruminal fermentation with Piper betle L. supplementation. Ciênc Rural 50:1–10
Purba RAP, C Yuangklang, S Paengkoum, P Paengkoum (2020d).
Milk fatty acid composition, rumen microbial population and animal performance
in response to diets rich in linoleic acid supplemented with Piper betle L. leaves in Saanen goats. Anim. Prod. Sci https://doi.org/10.1071/AN20182
Soest PJV, JB Robertson, BA Lewis (1991). Methods for
dietary fiber, neutral detergentfiber, andnonstarch polysaccharides in relation
to animal nutrition. J Dairy Sci
74:3583‒3597
Theodorou MK, BA Williams, MS Dhanoa, AB McAllan, J
France (1994). A simple gas production method using a pressure transducer to
determine the fermentation kinetics of ruminant feeds. Anim Feed Sci Technol 48:185‒197
Tian XZ, H Xin, P Paengkoum, S Paengkoum, C Ban, T
Sorasak (2018). Effects of anthocyanin-rich purple corn (Zea mays L.) stover silage on nutrient utilization, rumen
fermentation, plasma antioxidant capacity, and mammary gland gene expression in
dairy goats. J Anim Sci 97:1384‒1397
Ultee A, MHJ Bennik, R Moezelaar (2002). The phenolic
hydroxyl group of carvacrol is essential for action against the food-borne
pathogen Bacillus cereus. Appl Environ Microbiol 68:1561‒1568
Vargas JE, S Andrés, TJ Snelling, L López-Ferreras, DR
Yáñez-Ruíz, C García-Estrada, S López (2017). Effect of sunflower and marine
oils on ruminal microbiota, in vitro
fermentation and digesta fatty acid profile. Front Microbiol 8; Article 1124
Wanapat M, A Cherdthong, P Pakdee, S Wanapat (2008).
Manipulation of rumen ecology by dietary lemongrass (Cymbopogon citratus Stapf.)
powder supplementation. J Anim Sci
86:3497‒3503
Weirdt RD, E Coenen, B Vlaeminck, V Fievez, PVD Abbeele,
TVD Wiele (2013). A simulated mucus layer protects Lactobacillus reuteri from the inhibitory effects of linoleic acid.
Benef Microbes 4:299‒312
Wolin MJ (1979). The
rumen fermentation: A model for microbial interactions in anaerobic ecosystems.
In: Advances in Microbial Ecology, Vol. 3, pp:49‒77. Alexander M (Ed.).
Springer US, Boston, Massachusetts, USA