Skip to main content

Rumen microbial degradation of bromoform from red seaweed (Asparagopsis taxiformis) and the impact on rumen fermentation and methanogenic archaea



The red macroalgae Asparagopsis is an effective methanogenesis inhibitor due to the presence of halogenated methane (CH4) analogues, primarily bromoform (CHBr3). This study aimed to investigate the degradation process of CHBr3 from A. taxiformis in the rumen and whether this process is diet-dependent. An in vitro batch culture system was used according to a 2 × 2 factorial design, assessing two A. taxiformis inclusion rates [0 (CTL) and 2% DM diet (AT)] and two diets [high-concentrate (HC) and high-forage diet (HF)]. Incubations lasted for 72 h and samples of headspace and fermentation liquid were taken at 0, 0.5, 1, 3, 6, 8, 12, 16, 24, 48 and 72 h to assess the pattern of degradation of CHBr3 into dibromomethane (CH2Br2) and fermentation parameters. Additionally, an in vitro experiment with pure cultures of seven methanogens strains (Methanobrevibacter smithii, Methanobrevibacter ruminantium, Methanosphaera stadtmanae, Methanosarcina barkeri, Methanobrevibacter millerae, Methanothermobacter wolfei and Methanobacterium mobile) was conducted to test the effects of increasing concentrations of CHBr3 (0.4, 2, 10 and 50 µmol/L).


The addition of AT significantly decreased CH4 production (P = 0.002) and the acetate:propionate ratio (P = 0.003) during a 72-h incubation. The concentrations of CHBr3 showed a rapid decrease with nearly 90% degraded within the first 3 h of incubation. On the contrary, CH2Br2 concentration quickly increased during the first 6 h and then gradually decreased towards the end of the incubation. Neither CHBr3 degradation nor CH2Br2 synthesis were affected by the type of diet used as substrate, suggesting that the fermentation rate is not a driving factor involved in CHBr3 degradation. The in vitro culture of methanogens showed a dose-response effect of CHBr3 by inhibiting the growth of M. smithii, M. ruminantium, M. stadtmanae, M. barkeri, M. millerae, M. wolfei, and M. mobile.


The present work demonstrated that CHBr3 from A. taxiformis is quickly degraded to CH2Br2 in the rumen and that the fermentation rate promoted by different diets is not a driving factor involved in CHBr3 degradation.


The fermentation of carbohydrates in the forestomach of ruminants into volatile fatty acids (VFA) produces dihydrogen (H2) and carbon dioxide (CO2) as fermentation by-products, which are used by methanogenic archaea in the rumen to generate methane (CH4) [1]. The release of enteric CH4 into the atmosphere represents a negative impact on the environment as its global warming potential is 28–34 times that of CO2 over 20-year horizon, but also a loss of 2%–12% of the gross feed energy from the animal [2]. Both the contribution to greenhouse gas emissions and energy loss justify the need for nutritional strategies to reduce enteric CH4 emissions without affecting the efficiency of feed utilization and animal health.

Recent investigations have shown that the use of some feed additives or supplements may provide potent emissions reduction [3]. Among the feed additives, the latest studies have demonstrated the inhibitory potential of certain brown and red macroalgae, particularly the genus Asparagopsis, when tested in vitro [4,5,6], in sheep [7], beef cattle [8, 9], and dairy cows [10, 11]. These studies have reported a wide range of CH4 reduction percentages with Asparagopsis supplementation. A recent meta-analysis of the effects of feeding predominantly Asparagopsis to cattle found a 37% reduction in CH4 yield [12], which is similar to the reductions achieved by other methanogenesis inhibitors, such as 3-nitrooxypropanol (22% and 39%, respectively in beef and dairy cattle) [13]. Nevertheless, other recent studies that tested the efficacy of Asparagopsis have reported CH4 reductions up to 80% [8, 10].

The CH4 inhibition by Asparagopsis is due to the presence of halogenated methane analogues (HMAs), encapsulated into specialized gland cells until its release as a natural plant defence mechanism [14]. Bromoform (CHBr3) has been shown to be the most abundant HMA in Asparagopsis as its principal anti-methanogenic compound [15]. The most reported mechanism for the inhibitory activity of HMAs in ruminants is by reacting with reduced vitamin B12 of coenzyme M methyltransferase and inhibiting the cobamide-dependent methyl-transferase step of methanogenesis [16, 17]. However, HMAs have also been found to bind to nickel tetrapyrrole (cofactor F430) of methyl-coenzyme M reductase (MCR), thereby inhibiting the reductive release of CH4 from methyl-coenzyme M [18,19,20]. Asparagopsis taxiformis is currently considered one of the most promising species due to its high CHBr3 content [1 to 15.8 mg/g of biomass on a dry matter (DM) basis] [19] and thus its capability for decreasing CH4 production when added at low inclusion rates to forage- and grain-based diets, without negatively affecting daily feed intake, feed conversion efficiencies or rumen function [21]. However, the large variation in the anti-methanogenic effect could be due to the inclusion rate, CHBr3 content in the seaweed, the fibre content in the diet received by the animal or the composition of the rumen microbial community [22]. A thorough understanding of how these factors affect the efficacy of A. taxiformis in decreasing enteric CH4 emissions is essential for the implementation of this mitigation strategy across all the different ruminant production systems.

Bromoform is recognized as an animal carcinogen and has been associated with renal and liver toxicity [23]. However, previous studies have shown no accumulation of CHBr3 in animal tissues or milk, taken from beef cattle [8] and dairy cows [10, 11] which had been offered Asparagopsis at low inclusion rates. This suggests that CHBr3 may be metabolised in the rumen. In contrast, a recent study with no control animals and high inclusion rates of A. taxiformis suggested that CHBr3 may be excreted in urine and milk in dairy cows [24]. However, its concentration in milk was less than half the United States Environment Protection Agency (U.S. EPA) drinking water standard for CHBr3. The transfer of HMAs, including CHBr3, into ruminant-derived food products is largely determined by its potential degradation or modification in the rumen environment. Studies have demonstrated that methanogens have the capacity to metabolise HMAs in nature [25,26,27] because coenzyme M methyltransferase, and specially MCR, can reductively dehalogenate a range of HMAs [28], including CHBr3 [17]. However, there is currently no literature on the metabolic fate of brominated halomethanes in the ruminant digestive system and whether the diet received by the animal could have an effect in the HMA degradation process.

Based on experiments that have shown degradation of chlorinated hydrocarbons in vitro in anaerobic sludge [29] and reductive dehalogenation of carbon tetrachloride by cell suspensions of archaea Methanosarcina barkeri resulting in chloroform, methylene chloride, methyl chloride, and CH4 as intermediates [28], we hypothesised that rumen methanogenic archaea catalyse the dehalogenation of CHBr3 to dibromomethane (CH2Br2), then bromomethane (CH3Br), and finally CH4 and bromine radical (Br). Therefore, the aim of the present study was to describe the degradation pattern of the active compound CHBr3 from A. taxiformis using an in vitro rumen simulation model under two dietary conditions representing different rumen fermentation rates. Additionally, the sensitivity of the most relevant methanogen species to CHBr3 was evaluated in vitro using seven pure cultures of methanogenic strains.

Materials and methods

Exp. 1: In vitro batch culture incubation

Fresh alfalfa hay and barley grain were used as substrate for the incubations. They were ground with a hammer mill (220 v, type WRB 90 Lb/4P, Dietz-motoren KG, Eleckromotorenfabrik, Dettingen unter Teck, Germany) to pass through a 1-mm screen. Asparagopsis taxiformis was obtained from SeaExpert (Faial, Portugal) and its CHBr3 concentration was 6 mg/g DM. It was freeze-dried and ground using a laboratory mill (IKA All analytical mill, Staufen, Germany) to pass through a 1-mm screen. The mill equipment was previously cooled in liquid nitrogen to avoid overheating and damaging A. taxiformis chemical integrity. Afterwards, A. taxiformis was ground 2 × 30 s with a 30-s interval between cycles to cool the mill. Milled A. taxiformis was stored in an airtight recipient contained in a desiccator and kept at 4 °C. Dry matter (DM), organic matter (OM), crude protein (CP), ether extract (EE), neutral detergent fibre (NDF), acid detergent fibre (ADF) and acid detergent lignin (ADL) of the substrates and the algae were analysed as described in Arco-Pérez et al. [30]. Dry matter (method 934.01) and ash (or OM) (method 942.05) were determined according to AOAC (2005) [31]. The nitrogen values (AOAC method 990.03) were determined using the Dumas method (Leco TruSpec CN, St. Joseph, MI, USA) and converted to CP by multiplying by 6.25. Ether extract was measured by extraction with petroleum ether (AOAC method 920.39). The analyses of NDF and ADF were carried out according to Van Soest et al. [32] using an Ankom 220 fiber analyser unit (Ankom Technology Corp., Macedon, NY, USA), with α-amylase for NDF analysis in concentrate samples, while ADL was determined by solubilisation of cellulose with 72% sulfuric acid. The chemical composition of alfalfa hay, barley grain and A. taxiformis is presented in Table 1.

Table 1 Chemical composition of the substrates of the diet and Asparagopsis taxiformis used in Exp. 1

An in vitro batch culture incubation [33] was used to study the degradation of CHBr3 naturally present in A. taxiformis in the rumen microbial environment. Rumen fluid was collected from five Limousine cows, aged 12 to 14 months, from a commercial slaughterhouse in Granada (Spain). The cows were adapted to a total mixed diet with a 50:50 forage:concentrate ratio in DM basis. The rumen digesta was filtrated through a double layer of cheese cloth and mixed with pre-warmed incubation buffer (0.35 g/L NaHCO3, 0.04 g/L (NH4)HCO3) [34] in a 1:2 ratio. Thereafter, 50 mL of the solution were anaerobically dispensed to 120 mL Wheaton bottles containing 0.5 g DM of the experimental diet.

Two diets differing in forage:concentrate ratio were used as fermentation substrate: 1) one diet with high concentrate proportion (HC; alfalfa hay and barley grain in a 30:70 ratio in DM) to promote a quick fermentation rate; and 2) a second diet high in forage (HF; alfalfa hay and barley grain in a 70:30 ratio in DM) to promote a slower and more sustained microbial fermentation rate. The objective of using two different diets was to assess whether the different fermentation rates could affect the degradation pattern of CHBr3. Moreover, for each diet, the inclusion or not of A. taxiformis on the top of the diet was considered: 1) A. taxiformis supplemented at 0 of substrate on a DM basis (Control, CTL); and 2) A. taxiformis supplemented at 2% of substrate on a DM basis (AT). The inclusion rate of A. taxiformis at 2% was chosen based on the observed CH4 inhibition in a previous in vitro study [35]. The objective of using two different diets was to assess whether the different fermentation rates could affect the degradation pattern of CHBr3. A total of 220 Wheaton bottles were used according to the following design: A. taxiformis inclusion level (CTL and AT) × substrate (HC and HF) × 11 sampling times for each rumen inoculum (n = 5). Different sets of Wheaton bottles were incubated for 0, 0.5, 1, 3, 6, 8, 12, 16, 24, 48 and 72 h to assess the pattern of degradation of CHBr3 into secondary metabolites. Immediately after inoculation, bottles were sealed, gently mixed, and kept in an incubator at 39 ºC.

At each sampling time (0, 0.5, 1, 3, 6, 8, 12, 16, 24, 48 and 72 h), headspace gas pressure measurement and headspace gas and culture content collection were performed from each set of Wheaton bottles that corresponded to the designated sampling point. Gas pressure in the headspace was measured using a Wide Range Pressure Meter (Sper Scientific LTD, Scottsdale, AZ, USA) and the entire volume of headspace gas was collected in 250-mL PVDF gas-tight bags (Cole-Parmer Kynar, Vernon Hills, IL, USA) for CH4 and H2 analyses. To ensure the complete collection of headspace gas, a syringe connected to the pressure transducer was used to extract the gas until the pressure inside the bottle reached zero. The headspace gas from the remaining bottles was released at each point until their sampling time. Samples of 10 mL of liquid culture content were collected at each time point in GC-MS vials to quantify the concentration of halogenated compounds (CHBr3 and CH2Br2). In addition, 0.8 mL liquid samples were collected at the end of the incubation (72 h) and diluted in 0.8 mL of an acid solution (0.5 mol/L HCl, 20 g/L metaphosphoric acid containing 0.8 g/L of crotonic acid as internal standard) to determine VFA concentration and profile. All the samples were stored at −20 ºC immediately after sampling.

The concentrations of CH4 and H2 in the headspace gas samples were determined using a micro gas chromatography system (Agilent 490, Santa Clara, CA, USA) equipped with two column channels: a 10 m CP-Molsieve 5A column on Ar as carrier gas, and a 10 m CP-PoraPLOT U column on He as carrier gas, following a methodology adapted from Cluett et al. [36]. The system was calibrated using a certified standard gas mix (Messer Gases for Life, Tarragona, Spain) with the following composition: 1% H2, 3% O2, 20% CH4, 26% N2, 50% CO2. A volume of 10 mL from each sample was directly introduced from the gas bags to the micro GC, using the internal sampling pump. The analysis was performed three times for each individual sample. The GC analyses were carried out at the Instrumental Technical Services of the Estación Experimental del Zaidín (SIC-EEZ), CSIC, Granada, Spain. Gas production was calculated by transforming pressure measurements into volume units using the Ideal Gas Law under standard atmospheric pressure and 39 ºC.

Concentrations of individual VFA (acetate, propionate, isobutyrate, butyrate, isovalerate and valerate) were determined by a GC system coupled with a Flame Ionization Detector (Auto-System PerkinElmer, Norwalk, CT, USA) using a crosslinked 100% polyethylene glycol column (TRB-FFAP, 30 m × 0.53 mm i.d. × 1 µm film thickness, Teknokroma, Spain), as described in Arco-Pérez et al. [30]. One μL of each sample was injected, in split mode (20 mL/min). Nitrogen (1 mL/min) was used as carrier gas, and the injector and detector temperature were 260 °C and 275 °C, respectively. The column temperature was maintained at 100 °C for 1 min, increased at 15 °C/min up to 160 °C, remaining at this point for 1 min. The identification of VFA peaks was based on the retention time of the external standards, using crotonic acid as the internal standard for quantification. Standard curves were prepared by dilution (1:1) of the standard mixture in the same solution in which the rumen content samples were added.

The concentrations of CHBr3 and CH2Br2 were measured as described in Colomb et al. [37]. Samples were analysed by headspace solid-phase micro extraction (CTC Analytics PAL Combi-xt Autosampler, Zwingen, Switzerland) interfaced with two-dimensional gas chromatography and with time-of-flight mass spectrometry (Waters Micromass Quattro micro GC, Milford, MA, USA). Analyte detection took place with mass spectrometry in full scan mode with 500 scans/s. The determination of CHBr3 and CH2Br2 were carried out at the Centre for Scientific Instrumentation of the University of Granada (CIC-UGR), Spain.

Exp. 2: In vitro pure cultures of methanogenic archaea

The pure cultures of six ruminal methanogens strains (Methanobrevibacter smithii DSM 861, Methanobrevibacter ruminantium DSM 1093, Methanosphaera stadtmanae DSM 3091, Methanosarcina barkeri DSM 800, Methanobrevibacter millerae DSM 16643 and Methanobacterium mobile DSM 1539) and Methanothermobacter wolfei DSM 2970 were acquired from DSMZ-German Collection of microorganisms and cell culture. These species were selected to represent some of the most abundant methanogens in the rumen across the main phylogenetic clades [38]. Methanogens cultures were carried out in Hungate tubes with medium and growing conditions as specified by DSMZ for anaerobes. Culture media (119, 120, 161, 322), described in detail at DSMZ website (, were prepared anaerobically, aseptically and under an atmosphere consisting of 80% H2 and 20% CO2 in anaerobic chamber (Whitley DG250 Anaerobic Workstation, Don Whitley Scientific Limited, West Yorkshire, UK). For the inoculation, ampoules with the different pure cultures were handled within an anaerobic chamber and under an atmosphere consisting of 80% H2 and 20% CO2 as specified by DSMZ. Two Hungate tubes containing 5 mL of the corresponding specific medium of every strain were used for the following treatments: control (CTL; no treatment applied), 100 µmol/L 2-bromoethanesulphonate (BES), as positive control of inhibition used in previous works [39], and increasing concentrations of CHBr3 (0.4, 2, 10 and 50 µmol/L). The dose range was determined to include the inclusion rate of A. taxiformis used in Exp. 1 (2% DM diet which is equivalent to 40 µmol/L). The compounds BES and CHBr3 were obtained from Sigma-Aldrich (Merck KGaA, Darmstadt, Germany). Stock solutions of BES (100 µmol/L) and CHBr3 (50 µmol/L) were prepared and stored at 4 ºC.

Cultures were incubated for 14 d, and the corresponding treatment was applied on d 2. Three consecutive incubation batches were run (n = 3) with analytical duplicates for each treatment that were averaged. Pressurization with H2/CO2 gas in anaerobic chamber was applied to achieve 1 bar in the tubes’ headspace. Tubes were horizontally placed in a shaking incubator at 37 ºC at 120 r/min in the dark. Methanogen growth was followed by CH4 production [40]. On d 2, 4, 6, 8, 10, 12 and 14 of incubation, 0.5-mL samples of gas produced were taken and immediately injected in a flame ionization-detection GC (HP Hewlett 5890, Packard Series II, Waldbronn, Germany) using a 0.5-mL Sample-Lock syringe (Hamilton, Nevada, USA) for CH4 analysis [41]. The concentration of CH4 was determined using a standard curve generated by injecting different volumes of 99.9% pure CH4 pre and post the injection of samples. After that, H2/CO2 gas was added to each tube to maintain 1 bar pressure.

Statistical analyses

Before conducting the ANOVA, the assumptions of the normality and homogeneity of the variance for Exp. 1 and 2 were checked using the Shapiro–Wilk and the Bartlett’s tests, respectively. Results from in vitro batch cultures (Exp. 1) were statistically analysed by a 2 × 2 factorial ANOVA:

$${Y}_{ijk} = \mu + {R}_{i} + {D}_{j} + {(R \times D)}_{ij} + {A}_{k} + {e}_{ijk}\, (\mathrm{one\, for\, each\, time\, point})$$

Where Yijk represents the dependent, continuous variable, µ is the overall population mean, Ri is the fixed effect of the A. taxiformis inclusion rate (CTL vs. AT), Dj is the fixed effect of the diet (HC vs. HF), (R × D)ij represents the interaction term, Ak represents the random effect of the animal inocula (n = 5), and eijk is the residual error.

Results from methanogenic archaea pure cultures (Exp. 2) were statistically analysed by repeated measures as follows:

$${Y}_{ijk} = \mu + {C}_{i} + {T}_{j} + {(C \times T)}_{ij} + {A}_{k} + {e}_{ijk}\, (\mathrm{one\, for\, each\, archaea\, pure\, culture})$$

Where Yijk represents the dependent, continuous variable, µ is the overall population mean, Ci is the fixed effect of CHBr3 concentration (0, 0.4, 2, 10, 50 µmol/L), Tj is the fixed effect of the time (2, 4, 6, 8, 10, 12 and 14 d), (C × T)ij represents the interaction term, Ak represents the repeated run (n = 3), and eijk is the residual error.

When significant effects were detected, polynomial contrasts were used to determine linear (L) and/or quadratic (Q) responses in Exp. 2, and means were compared by Fisher’s protected LSD test when significant interactions were found (P < 0.05), using the StatGraphics Centurion 19 software (StatPoint Technologies, Inc. USA, 2020). Significant effects were declared at P < 0.05 and tendencies to differences at P < 0.10.


Exp. 1: In vitro batch culture incubation

Fermentation profile

The results from the in vitro gas production test confirmed that different fermentation pattern was obtained by using either HC or HF diets (Table 2). This was reflected not only in significantly greater volume of gas produced by HC diet (P = 0.046) but also a significantly greater gas production rate (P = 0.046) at most time intervals. No significant differences were noted in total VFA production (P = 0.243), but the HC diet promoted a higher molar proportion of propionate (P = 0.001), butyrate (P = 0.008) and valerate (P = 0.021), whereas the HF diet promoted a higher acetate molar proportion (P < 0.001) (Table 3).

Table 2 Effect of the inclusion rate (R) of Asparagopsis taxiformis and the type of diet (D) on the in vitro cumulative gas production and production rate at different incubation intervals (Exp. 1)
Table 3 Effect of the inclusion rate (R) of Asparagopsis taxiformis and the type of diet (D) on rumen fermentation parameters at 72 h of incubation (Exp. 1)

The addition of AT significantly decreased the cumulative gas production (Table 2) at every time interval (P < 0.001), but not the VFA production (Table 3) after 72 h incubation (P = 0.446). Additionally, AT treatment had a strong effect on fermentation pattern promoting an increase in the molar proportions of propionate, butyrate and valerate (P < 0.001), and a decrease in the molar proportion of acetate (P < 0.001).

Table 3 also shows a significant interaction (P = 0.003) between A. taxiformis inclusion rate and the type of diet (R × D) for the acetate:propionate ratio (A:P) indicating a larger decrease for the HF than for the HC diet.

Methane and dihydrogen production

The main effect of AT inclusion on rumen fermentation was reflected in a substantial inhibition of CH4 cumulative production (P = 0.002) and production rate (P = 0.018) for both diets from 1.5 to 72 h of incubation (Table 4). During the initial incubation period (0–1.5 h), a significant interaction (P = 0.029) showed that the inhibition of CH4 cumulative production and production rate were only detected with the HF diet.

Table 4 Effect of the inclusion rate (R) of Asparagopsis taxiformis and the type of diet (D) on the in vitro CH4 cumulative production and production rate at different incubation intervals (Exp. 1)

This strong inhibition of methanogenesis resulted in increased H2 production rate, which was significantly higher (P = 0.006) in AT than in CTL from 1.5 to 12 h of incubation (Table 5). Hydrogen cumulative production was significantly increased (P = 0.020) for HC compared to HF diet at 12 h of incubation. From 24 h until the end of the incubation period, the effect of AT on H2 cumulative production significantly differed (significant interaction, P < 0.032) based on the type of diet, with a greater increase observed when AT was included with HC diet.

Table 5 Effect of the inclusion rate (R) of Asparagopsis taxiformis and the type of diet (D) on the in vitro H2 cumulative production and production rate at different incubation intervals (Exp. 1)

Bromoform degradation pattern

The monitorization of CHBr3 and CH2Br2 concentrations throughout the incubation process is showed in Fig. 1. A rapid degradation of CHBr3 was observed, with 70% degraded within the first 30 min and nearly 90% after 3 h of incubation. Most (> 99%) of the CHBr3 was degraded within 12 h of incubation.

Fig. 1
figure 1

Effect of supplementing with Asparagopsis taxiformis at 2% DM (AT) to high-concentrate (HC) and high-forage (HF) diets on the in vitro concentration (mmol/L) of bromoform (CHBr3) and dibromomethane (CH2Br2) at different incubation times (h)

In line with the observations on CHBr3 degradation, CH2Br2 was not detected at 0 h but its presence was quickly detected in the samples after the incubation began and increasing rapidly until it peaked at 6–8 h of incubation. Then, a gradual decline in concentration was observed towards the end of the incubation period (18 to 72 h) at which around 50% of the maximum CH2Br2 detected at 6 h was no longer present in the samples. Neither CHBr3 degradation nor CH2Br2 synthesis were significantly affected by the type of diet used as substrate (HC or HF).

Exp. 2: In vitro pure cultures of methanogenic archaea

The increasing addition of CHBr3 promoted a quadratic response in the inhibition of the growth of M. smithii, M. ruminantium, M. stadtmanae, M. millerae, M. wolfei, and M. mobile, with the highest drop observed for concentrations between 2 and 10 µmol/L, depending on the methanogens species. Moreover, a linear dose-response was observed for M. barkeri (Table 6; Fig. 2). Methanosphaera stadtmanae (Fig. 2C) and M. ruminantium (Fig. 2C) were the most affected strains to the highest concentrations of CHBr3 (50 µmol/L), while M. smithii (Fig. 2A) and M. mobile (Fig. 2G) could be considered the most resistant species to the anti-methanogenic activity of CHBr3, as their growing rates were only decreased by around 30%. The incubation time also modulated the CH4 inhibition promoting a linear decrease for M. smithii and linear increases for M. ruminantium and M. barkeri, while quadratic responses were noted for M. stadtmanae and M. millerae.

Table 6 Effect of bromoform at different concentrations (C) and incubation times (T) on CH4 inhibition rate (%) in different archaeal species (Exp. 2)
Fig. 2
figure 2

Effect of bromoform (CH3Br) at different concentrations (0.4, 2, 10 and 50 µmol/L) on the growth (mL CH4/mL gas) of Methanobrevibacter smithii (A), Methanobrevibacter ruminantium (B), Methanosphaera stadtmanae (C), Methanosarcina barkeri (D), Methanobrevibacter millerae (E) Methanothermobacter wolfei (F) and Methanobacterium mobile (G)


Microbial fermentation profile

The type of diet consumed by the ruminant, and particularly the forage:concentrate ratio, determines to a great extent the fermentation pattern in the rumen [42]. There is a faster fermentation rate of carbohydrates when the proportion of concentrate in the diet is increased, whereas diets mainly based on forage have a high content in structural carbohydrates such as cellulose and hemicellulose, which require longer times to be degraded by rumen microorganisms. Our study showed that HC diet resulted in a greater volume of gas produced compared with HF diet, suggesting a greater yield of fermentation products when concentrate proportion is increased [43]. The differences between diets were reflected in a shift in A:P and the fermentation rate. A greater supply of fermentable carbohydrates leads to a faster fermentation rate, increasing microbial growth and thus enhancing the degradation potential of different substrates. Hagemeister et al. [44] showed an increase of 22.1 g of microbial protein biomass per 100 g increase in fermentable organic matter supplied to the rumen.

According to Roque et al. [45], the inclusion of AT had an effect on in vitro cumulative gas production. In our study, the efficacy of AT to decrease the volume of gas produced was detected at the beginning of the fermentation and remained consistent during the 72 h incubation period. Our results differ with those from Machado et al. [46] since AT did not decrease total VFA production. This discrepancy could be explained by the far greater level of inclusion used by Machado et al. [46], which reached up to 16.7% of total OM in the diet. However, both studies agree with the finding that AT changed the VFA profile. Acetate molar proportion decreased whereas that of propionate and butyrate increased, decreasing A:P as reported by Roque et al. [45], Machado et al. [46] and Kinley et al. [47]. When methanogenesis is inhibited, an increase in propionate production is normally observed because pyruvate is reduced to propionate in one of two multi-step pathways [48].


Consistent with previous works [7,8,9, 11], the present study demonstrated the anti-methanogenic activity of A. taxiformis. The 97% reduction of CH4 production was similar to the level of reduction observed in a previous in vitro study with the same batch of A. taxiformis and inclusion rate [35]. Machado et al. [46] reported 85% reduction of CH4 production with 1% (OM basis) inclusion rate in the diet and a nearly total reduction at doses above 2%. Kinley et al. [47] observed that no detectable CH4 was produced with 2% (OM basis) A. taxiformis inclusion after 24 h. Roque et al. [45] reported a 95% reduction in CH4 production when the dosage was increased to 5% OM. It is noticeable that the literature reflects that the methanogenesis inhibition rate achieved by the addition of AT is rather variable, which could potentially be due to different factors such as differences in AT inclusion rate, animal species, diet formulation and CHBr3 content of the macroalgae, which in turn depends on its geographical origin, harvesting season and storage conditions [22].

As described above, the lower forage:concentrate ratio in the diet shifted the fermentation profile from acetate towards propionate production. As the proportion of forage in the diet increases, the proportion of acetate rises and propionate decreases, which means a displacement from H2-incorporating propionate to H2-producing acetate production [49]. Whereas higher dietary content of fibre increases H2 formation, promoting the methanogenic activity of rumen archaea, diets with higher content of starch deprive methanogens of H2 and thus decrease CH4 production [50].

Dihydrogen formation

The substantial reduction of CH4 production by the addition of AT was accompanied by an increase in rumen H2 accumulation, in agreement with previous studies that used AT [8, 9] and other anti-methanogenic feed additives [51, 52]. Elevation of H2 was expected as methanogenesis is the main metabolic H2 sink in the rumen. When CH4 production is inhibited, rumen H2 partial pressure increases and, above a certain threshold, rumen fermentation can be potentially compromised [53]. There are regulatory mechanisms to avoid rumen excess H2, which involve redirecting part of it towards alternative metabolic pathways such as H2-incorporating propionate production [54]. This could explain the alteration of A:P previously observed in this study. However, the propionate production pathway was not efficient enough to capture all the available H2 that otherwise would be utilised for the production of CH4, and most of the excess H2 was then released into the gas phase. This observation suggests that there is still room for developing strategies to capture this H2 into valuable fermentation products for the ruminant.

Interestingly, the H2 production was also influenced by the type of diet after 12 h of fermentation. Greater amounts of H2 were induced by HC diet compared to HF diet. This agrees with Vyas et al. [52] that showed greater emissions of H2 by methanogenesis-inhibited animals fed HC diet compared with a mixed forage:concentrate diet. According to Martinez-Fernandez et al. [55], the rumen microbiota utilised more H2 available from methanogenesis inhibition when the proportion of forage in the diet was increased. This is possibly due to the slower fermentation rate of the HF diet which might allow a more efficient utilisation of the H2 released, compared with the highly fermentable HC diet which might produce H2 faster than the rumen methanogens are able to consume.

Bromoform degradation

Bromoform is the most abundant halogenated metabolite in A. taxiformis that provides anti-methanogenic activity to the macroalgae [15]. For A. taxiformis to be considered a practical tool for CH4 production mitigation, it is essential to guarantee that food products from livestock fed the macroalgae are safe for consumption and that elevated CHBr3 levels are not detected in animal tissues or products. No CHBr3 residues have been found in samples of kidney, liver, faeces, fat, muscle tissue or milk taken from sheep [7] and beef cattle [8, 9] fed diets with AT at inclusion levels from 0.2% to 1% DM. This suggests that CHBr3 is either degraded in the digestive tract or, if absorbed into the animal tissues, is converted to other metabolites.

As reviewed by Glasson et al. [19], studies with methanogens have demonstrated that coenzyme M methyltransferase and MCR reductively dehalogenate a range of HMAs to CH4 and other less halogenated intermediates, with cofactor F430 of MCR 50 times more active than coenzyme M methyltransferase [28]. The efficiency of HMA dehalogenation also increases according to expected carbon-halogen bond dissociation energies which decrease in the order F > Cl > Br > I. Therefore, CHBr3 would be more efficiently dehalogenated than chloroform. Based on Van Eekert et al. [29] that described chlorinated degradation in vitro in anaerobic sludge, we hypothesized that CHBr3 was degraded to CH2Br2, then CH3Br, and finally CH4 and Br. Our work demonstrated the dehalogenation process of CHBr3 to CH2Br2 by rumen microbes. We observed that more than 3 mmol/L CHBr3 were degraded within 30 min, whereas CH2Br2 only reached a concentration of 0.4 mmol/L by 30 min and never reached a concentration higher than 1.2 mmol/L in both diets. This suggests that either CHBr3 is being degraded through a non-CH2Br2 pathway or that CH2Br2 generated over the first 30 min had an extremely short half-life and the experimental approach used was not able to detect its production. The latter conclusion would be consistent with a degradation mechanism that significantly depleted cofactor F430 within the first 30 min of fermentation, resulting in a long-term inhibition of CH4 production and a long residence time for HMA in the latter hours of the experiment. Cofactor F430 is an essential prosthetic group of MCR, which catalyses the last step of methanogenesis [27]. In the actual rumen environment, some amount of F430 regeneration would be expected, as would complete degradation of the HMAs. The lack of detection of CH3Br and Br as intermediate and end-product of the degradation process, respectively, might be explained by the high volatility of CH3Br and the high reactivity of Br with different compounds under the rumen fermentation conditions and the difficulty to use a samples collection procedure from the fermentation vessels to ensure their detection. This deserves further analytical evaluation in future studies.

Our results showed that neither CHBr3 degradation nor CH2Br2 synthesis were significantly affected by the type of diet used as substrate, suggesting that the overall rumen fermentation rate is not a driving factor involved in CHBr3 degradation, therefore, similar conclusions can be achieved regardless the diet used by the animal.

Further in vivo investigations are needed to validate the suggested pathway for CHBr3 degradation in the rumen. The inclusion rate of A. taxiformis should be adjusted to in vivo conditions, as it should not exceed 1% DM due to reductions in feed intake at higher inclusion levels [10, 11]. Considering the rapid degradation of CHBr3 observed in vitro and the longer residence time of the digesta in the rumen [56], it is likely that the same results would be observed in vivo. If this is confirmed in vivo, it would provide evidence that CHBr3 undergoes rapid degradation upon administration in the rumen, and therefore would not be transferred to animal tissues, milk or urine.

Methanogenic archaea

Rumen methanogens are microbes capable of producing energy through the reduction of CO2 to CH4 with consumption of H2 from anaerobic fermentation [1]. Mitigation strategies based on the use of HMAs, such as CHBr3, whose mechanism of action consists of directly blocking one or more steps of the methanogenic process, are depriving methanogens of their main source of energy [54]. Therefore, inhibition of methanogenesis potentially leads to a reduction in the growth of methanogenic archaeal population [57]. In vitro trials reported significant decreases of the abundance of methanogens with the inclusion of A. taxiformis [45, 58] or others synthetic HMA inhibitors [55, 59]. However, the rumen methanogens population is diverse and variable [60] and not all species might be equally sensitive to CHBr3 as the key active compound of A. taxiformis.

Pure cultures of seven strains of methanogenic archaea, six representing some of the most abundant in the rumen, were used in the present study to evaluate the impact of increasing doses of CHBr3 on their individual growth. The minimum concentration tested (0.4 µmol/L CHBr3) was sufficient to decrease the growth of all species but not at the same reduction level. For instance, the growth of M. ruminantium and M. stadtmanae were reduced by more than 50% at that dosage. Previous studies [39, 61] reported the high sensitivity of M. ruminantium to BES, another specific inhibitor of the last step of the methanogenesis pathway. However, no significant decrease in M. ruminantium growth was observed when CHBr3 concentration was further increased. Conversely, M. smithii, M. stadtmanae, M. barkeri, M. millerae, M. wolfei and M. mobile growing rates were affected in a dose-dependent manner, reaching different rates of CH4 inhibition as level of inclusion of CHBr3 increased. Both M. mobile and M. smithii could be considered the most resistant strains to CHBr3 as their growing rate was less affected than the others. Similar differences among methanogenic archaea species in response to 3-nitrooxypropanol supplementation were observed by Duin et al. [62].

Differences in the sensitiveness of methanogenic archaea to methanogenesis inhibitors have been attributed to some extent to the varying ability to uptake these inhibitors into the cells [63]. The genus Methanobrevibacter, which is the most dominant member of the rumen archaeal community, can be divided into two subgroups according to their expression of MCR that catalyses the rate limiting step of methanogenesis [64]. Methanobrevibacter smithii belongs to the clade capable of synthesising both forms of MCR (MCRI and MCRII) while M. ruminantium only possesses MCRI [65]. Therefore, M. ruminantium methanogenesis pathway is more limited and can be more rapidly blocked by HMA inhibitors, while M. smithii has greater MCR activity and requires a higher concentration of inhibitors such as CHBr3 to be strongly affected. For the rest of methanogens studied here, it could be suggested that their sensitivity may depend on the saturation capacity of their MCR enzymatic system. Further research on MCR specific characteristics of other species could help to fully understand the impact that CHBr3 has on the rumen archaeal population.

Furthermore, the composition of the rumen methanogens community is largely influenced by the basal diet, ruminant species, management, and geographical area [60]. Therefore, it could be expected that the variable relative abundance of the different species of methanogens in the rumen ecosystem, as a consequence of the above listed factors, determined the inhibitory potential of CHBr3 containing additives. Consequently, variations in all of these factors could indirectly affect the CH4 inhibition rate reached by mitigation strategies based on A. taxiformis supplementation. A complete understanding of the rumen microbiome in response to A. taxiformis supplementation in animals under different dietary conditions may allow accurate predictions of treatment efficacy.


Our results show that under in vitro conditions CHBr3 is quickly degraded in the rumen, with 90% broken down within the first 3 h. The diet used as substrate does affect neither CHBr3 degradation nor CH2Br2 synthesis, suggesting the fermentation rate is not a driving factor involved in CHBr3 degradation. Using pure cultures, CHBr3 is shown to inhibit the growth of methanogenic archaea at very low concentrations with some differences among species, which deserve more research to fully understand the potential effectiveness across different dietary regimes. These findings can help to uncover the mode of action of the dietary supplementation with A. taxiformis as one of the most promising CH4 mitigation strategies in ruminant production.

Availability of data and materials

All data generated and/or analysed during the current study are available from the corresponding author on reasonable request.



Acid detergent fibre


Acid detergent lignin


Acetate:propionate ratio


Asparagopsis taxiformis at 2% DM





CHBr3 :


CH2Br2 :




CH4 :


CO2 :

Carbon dioxide


Crude protein


Control (Asparagopsis taxiformis at 0 DM)


Dry matter


Ether extract

H2 :



High-concentrate diet


High-forage diet


Halogenated methane analogues


Methyl-coenzyme M reductase


Neutral detergent fibre


Organic matter


Standard error of the mean


Volatile fatty acids


  1. Moss AR, Jouany JP, Newbold J. Methane production by ruminants: its contribution to global warming. Ann Zootech. 2000;49(3):231–53.

    Article  CAS  Google Scholar 

  2. Johnson KA, Johnson DE. Methane emissions from cattle. J Anim Sci. 1995;73(8):2483–92.

    Article  CAS  PubMed  Google Scholar 

  3. Arndt C, Hristov AN, Price WJ, McClelland SC, Pelaez AM, Cueva SF, et al. Full adoption of the most effective strategies to mitigate methane emissions by ruminants can help meet the 1.5 °C target by 2030 but not 2050. Proc Natl Acad Sci U S A. 2022;119(20):e2111294119.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  4. Brooke CG, Roque BM, Shaw C, Najafi N, Gonzalez M, Pfefferlen A, et al. Methane reduction potential of two pacific coast macroalgae during in vitro ruminant fermentation. Front Mar Sci. 2020;7:561.

    Article  Google Scholar 

  5. Machado L, Magnusson M, Paul NA, de Nys R, Tomkins N. Effects of marine and freshwater macroalgae on in vitro total gas and methane production. PLoS One. 2014;9(1):e85289.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  6. Maia MRG, Fonseca AJM, Oliveira HM, Mendonca C, Cabrita ARJ. The potential role of seaweeds in the natural manipulation of rumen fermentation and methane production. Sci Rep. 2016;6:32321.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  7. Li X, Norman HC, Kinley RD, Laurence M, Wilmot M, Bender H, et al. Asparagopsis taxiformis decreases enteric methane production from sheep. Anim Prod Sci. 2016;58(4):681–8.

    Article  CAS  Google Scholar 

  8. Kinley RD, Martinez-Fernandez G, Matthews MK, de Nys R, Magnusson M, Tomkins NW. Mitigating the carbon footprint and improving productivity of ruminant livestock agriculture using a red seaweed. J Clean Prod. 2020;259:120836.

    Article  Google Scholar 

  9. Roque BM, Venegas M, Kinley RD, de Nys R, Duarte TL, Yang X, et al. Red seaweed (Asparagopsis taxiformis) supplementation reduces enteric methane by over 80 percent in beef steers. PLoS One. 2021;16(3):e0247820.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  10. Roque BM, Salwen JK, Kinley R, Kebreab E. Inclusion of Asparagopsis armata in lactating dairy cows’ diet reduces enteric methane emission by over 50 percent. J Clean Prod. 2019;234:132–8.

    Article  CAS  Google Scholar 

  11. Stefenoni HA, Räisänen SE, Cueva SF, Wasson DE, Lage CFA, Melgar A, et al. Effects of the macroalga Asparagopsis taxiformis and oregano leaves on methane emission, rumen fermentation, and lactational performance of dairy cows. J Dairy Sci. 2021;104(4):4157–73.

    Article  CAS  PubMed  Google Scholar 

  12. Lean IJ, Golder HM, Grant TMD, Moate PJ. A meta-analysis of effects of dietary seaweed on beef and dairy cattle performance and methane yield. PLoS One. 2021;16(7):e0249053.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  13. Dijkstra J, Bannink A, France J, Kebreab E, van Gastelen S. Antimethanogenic effects of 3-nitrooxypropanol depend on supplementation dose, dietary fiber content, and cattle type. J Dairy Sci. 2018;101(10):9041–7.

    Article  CAS  PubMed  Google Scholar 

  14. Paul NA, de Nys R, Steinberg PD. Chemical defence against bacteria in the red alga Asparagopsis armata: linking structure with function. Mar Ecol Prog Ser. 2006;306:87–101.

    Article  CAS  Google Scholar 

  15. Machado L, Magnusson M, Paul NA, Kinley R, de Nys R, Tomkins N. Identification of bioactives from the red seaweed Asparagopsis taxiformis that promote antimethanogenic activity in vitro. J Appl Phycol. 2016;28(5):3117–26.

    Article  CAS  Google Scholar 

  16. Honan M, Feng X, Tricarico JM, Kebreab E. Feed additives as a strategic approach to reduce enteric methane production in cattle: modes of action, effectiveness and safety. Anim Prod Sci. 2021;62:1303–17.

    Article  CAS  Google Scholar 

  17. Wood JM, Kennedy FS, Wolfe RS. The reaction of multihalogenated hydrocarbons with free and bound reduced vitamin B12. Biochemistry. 1968;7(5):1707–13.

    Article  CAS  PubMed  Google Scholar 

  18. Ermler U. On the mechanism of methyl-coenzyme M reductase. Dalton Trans. 2005;21:3451–8.

    Article  CAS  Google Scholar 

  19. Glasson CRK, Kinley RD, de Nys R, King N, Adams SL, Packer MA, et al. Benefits and risks of including the bromoform containing seaweed Asparagopsis in feed for the reduction of methane production from ruminants. Algal Res. 2022;64:102673.

    Article  Google Scholar 

  20. Yang N, Reiher M, Wang M, Harmer J, Duin EC. Formation of a nickel-methyl species in methyl-coenzyme m reductase, an enzyme catalyzing methane formation. J Am Chem Soc. 2007;129(36):11028–9.

    Article  CAS  PubMed  Google Scholar 

  21. Min BR, Parker D, Brauer D, Waldrip H, Lockard C, Hales K, et al. The role of seaweed as a potential dietary supplementation for enteric methane mitigation in ruminants: challenges and opportunities. Anim Nutr. 2021;7(4):1371–87.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  22. Hegarty RS, Passetti RAC, Dittmer KM, Wang Y, Shelton S, Emmet-Booth J, et al. An evaluation of evidence for efficacy and applicability of methane inhibiting feed additives for livestock. Consultative Group for International Agricultural Research (CGIAR); 2021. Accessed 1 Dec 2021.

  23. Condie LW, Smallwood CL, Laurie RD. Comparative renal and hepatotoxicity of halomethanes: bromodichloromethane, bromoform, chloroform, dibromochloromethane and methylene chloride. Drug Chem Toxicol. 1983;6(6):563–78.

    Article  CAS  PubMed  Google Scholar 

  24. Muizelaar W, Groot M, van Duinkerken G, Peters R, Dijkstra J. Safety and transfer study: transfer of bromoform present in Asparagopsis taxiformis to milk and urine of lactating dairy cows. Foods. 2021;10(3):584.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  25. Guo M, Chen Y. Coenzyme cobalamin: biosynthesis, overproduction and its application in dehalogenation—a review. Rev Environ Sci Biotechnol. 2018;17:259–84.

    Article  CAS  Google Scholar 

  26. Holliger C, Schraa G, Stupperich E, Stams AJ, Zehnder AJ. Evidence for the involvement of corrinoids and factor F430 in the reductive dechlorination of 1,2-dichloroethane by Methanosarcina barkeri. J Bacteriol. 1992;174(13):4427–34.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  27. Jaun B, Thauer RK. Methyl-coenzyme M reductase and its nickel corphin coenzyme F430 in methanogenic archaea. In: Sigel A, Sigel H, Sigel RKO, editors. Nickel and its surprising impact in nature, vol. 2. New Jersey: Wiley; 2007. p. 323–56.

    Chapter  Google Scholar 

  28. Krone UE, Laufer K, Thauer RK, Hogenkamp HP. Coenzyme F430 as a possible catalyst for the reductive dehalogenation of chlorinated C1 hydrocarbons in methanogenic bacteria. Biochemistry. 1989;28(26):10061–5.

    Article  CAS  PubMed  Google Scholar 

  29. Van Eekert MHA, Schröder TJ, Stams AJM, Schraa G, Field JA. Degradation and fate of carbon tetrachloride in unadapted methanogenic granular sludge. Appl Environ Microbiol. 1998;64(7):2350–6.

    Article  PubMed Central  Google Scholar 

  30. Arco-Pérez A, Ramos-Morales E, Yáñez-Ruiz DR, Abecia L, Martín-García AI. Nutritive evaluation and milk quality of including of tomato or olive by-products silages with sunflower oil in the diet of dairy goats. Anim Feed Sci Technol. 2017;232:57–70.

    Article  CAS  Google Scholar 

  31. AOAC. Official methods of analysis of AOAC International. 18th ed. In: Horwitz W, editor. Gaithersberg: AOAC International; 2005.

  32. 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(10):3583–97.

    Article  PubMed  Google Scholar 

  33. Yáñez-Ruiz DR, Bannink A, Dijkstra J, Kebreab E, Morgavi DP, O’Kiely P, et al. Design, implementation and interpretation of in vitro batch culture experiments to assess enteric methane mitigation in ruminants – a review. Anim Feed Sci Technol. 2016;216:1–18.

    Article  CAS  Google Scholar 

  34. Mould FL, Morgan R, Kliem KE, Krystallidou E. A review and simplification of the in vitro incubation medium. Anim Feed Sci Technol. 2005;123–124:155–72.

    Article  Google Scholar 

  35. Romero P, Huang R, Jiménez E, Palma-Hildalgo JM, Ungerfeld EM, Popova M, et al. Evaluating the effect of phenolic compounds as hydrogen acceptors when ruminal methanogenesis is inhibited in vitro – part 2. Dairy goats. Animal. 2023;17(5):100789.

    Article  CAS  PubMed  Google Scholar 

  36. Cluett J, VanderZaag AC, Balde H, McGinn S, Jenson E, Hayes AC, et al. Effects of two manure additives on methane emissions from dairy manure. Animals. 2020;10(5):807.

    Article  Google Scholar 

  37. Colomb A, Yassaa N, Williams J, Peeken I, Lochte K. Screening volatile organic compounds (VOCs) emissions from five marine phytoplankton species by head space gas chromatography/mass spectrometry (HS-GC/MS). J Environ Monit. 2008;10(3):325–30.

    Article  CAS  PubMed  Google Scholar 

  38. Snelling TJ, Genç B, McKain N, Watson M, Waters SM, Creevey CJ, et al. Diversity and community composition of methanogenic archaea in the rumen of Scottish upland sheep assessed by different methods. PLoS One. 2014;9(9):e106491.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  39. Ungerfeld EM, Rust SR, Boone DR, Liu Y. Effects of several inhibitors on pure cultures of ruminal methanogens. J Appl Microbiol. 2004;97(3):520–6.

    Article  CAS  PubMed  Google Scholar 

  40. Balch WE, Wolfe RS. New approach to the cultivation of methanogenic bacteria: 2-mercaptoethanesulfonic acid (HS-CoM)-dependent growth of Methanobacterium ruminantium in a pressureized atmosphere. Appl Environ Microbiol. 1976;32(6):781–91.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  41. Chong SC, Liu Y, Cummins M, Valentine DL, Boone DR. Methanogenium marinum sp. nov., a H2-using methanogen from Skan Bay, Alaska, and kinetics of H2 utilization. Antonie Van Leeuwenhoek. 2002;81(1–4):263–70.

    Article  CAS  PubMed  Google Scholar 

  42. 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.

    Article  CAS  Google Scholar 

  43. Belanche A, Palma-Hidalgo JM, Nejjam I, Serrano R, Jiménez E, Martín-García I, et al. In vitro assessment of the factors that determine the activity of the rumen microbiota for further applications as inoculum. J Sci Food Agric. 2019;99(1):163–72.

    Article  CAS  PubMed  Google Scholar 

  44. Hagemeister H, Liipping W, Kaufmann W. Microbial protein synthesis and digestion in the high-yielding dairy cow. In: Haresign W, Cole DJA, editors. Recent developments in ruminant nutrition. London: Elsevier; 1981. p. 31–48.

    Chapter  Google Scholar 

  45. Roque BM, Brooke CG, Ladau J, Polley T, Marsh LJ, Najafi N, et al. Effect of the macroalgae Asparagopsis taxiformis on methane production and rumen microbiome assemblage. Anim Microbiome. 2019;1(1):3.

    Article  PubMed  PubMed Central  Google Scholar 

  46. Machado L, Magnusson M, Paul NA, Kinley R, de Nys R, Tomkins N. Dose-response effects of Asparagopsis taxiformis and Oedogonium sp. on in vitro fermentation and methane production. J Appl Phycol. 2016;28(2):1443–52.

    Article  CAS  Google Scholar 

  47. Kinley RD, de Nys R, Vucko MJ, Machado L, Tomkins NW. The red macroalgae Asparagopsis taxiformis is a potent natural antimethanogenic that reduces methane production during in vitro fermentation with rumen fluid. Anim Prod Sci. 2016;56(3):282–9.

    Article  CAS  Google Scholar 

  48. Baldwin RL, Wood WA, Emery RS. Conversion of glucose-C14 to propionate by the rumen microbiota. J Bacteriol. 1963;85(6):1346–9.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  49. Wang L, Zhang G, Li Y, Zhang Y. Effects of high forage/concentrate diet on volatile fatty acid production and the microorganisms involved in VFA production in cow rumen. Animals (Basel). 2020;10(2):223.

    Article  PubMed  Google Scholar 

  50. Valadares RFD, Broderick GA, Valadares Filho SC, Clayton MK. Effect of replacing alfalfa silage with high moisture corn on ruminal protein synthesis estimated from excretion of total purine derivatives. J Dairy Sci. 1999;82(12):2686–96.

    Article  CAS  PubMed  Google Scholar 

  51. Hristov AN, Oh J, Giallongo F, Frederick TW, Harper MT, Weeks HL, et al. An inhibitor persistently decreased enteric methane emission from dairy cows with no negative effect on milk production. Proc Natl Acad Sci U S A. 2015;112(34):10663–8.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  52. Vyas D, McGinn SM, Duval SM, Kindermann MK, Beauchemin KA. Optimal dose of 3-nitrooxypropanol for decreasing enteric methane emissions from beef cattle fed high-forage and high-grain diets. Anim Prod Sci. 2016;58(6):1049–55.

    Article  CAS  Google Scholar 

  53. Wolin MJ, Miller TL, Stewart CS. Microbe-microbe interactions. In: Hobson PN, Stewart CS, editors. The rumen microbial ecosystem. New York: Blackie Academic and Professional; 1997. p. 467–91.

    Chapter  Google Scholar 

  54. Janssen PH. Influence of hydrogen on rumen methane formation and fermentation balances through microbial growth kinetics and fermentation thermodynamics. Anim Feed Sci Technol. 2010;160(1–2):1–22.

    Article  CAS  Google Scholar 

  55. Martinez-Fernandez G, Denman SE, Yang C, Cheung J, Mitsumori M, Mcsweeney CS. Methane inhibition alters the microbial community, hydrogen flow, and fermentation response in the rumen of cattle. Front Microbiol. 2016;7:1122.

    Article  PubMed  PubMed Central  Google Scholar 

  56. Mambrini M, Peyraud JL. Retention time of feed particles and liquids in the stomachs and intestines of dairy cows. Direct measurement and calculations based on faecal collection. Reprod Nutr Dev. 1997;37(4):427–42.

    Article  CAS  PubMed  Google Scholar 

  57. Denman SE, Martinez Fernandez G, Shinkai T, Mitsumori M, McSweeney CS. Metagenomic analysis of the rumen microbial community following inhibition of methane formation by a halogenated methane analog. Front Microbiol. 2015;6:1087.

    Article  PubMed  PubMed Central  Google Scholar 

  58. Machado L, Tomkins N, Magnusson M, Midgley DJ, de Nys R, Rosewarne CP. In vitro response of rumen microbiota to the antimethanogenic red macroalga Asparagopsis taxiformis. Microb Ecol. 2018;75(3):811–8.

    Article  PubMed  Google Scholar 

  59. Martinez-Fernandez G, Denman SE, Cheung J, McSweeney CS. Phloroglucinol degradation in the rumen promotes the capture of excess hydrogen generated from methanogenesis inhibition. Front Microbiol. 2017;8:1871.

    Article  PubMed  PubMed Central  Google Scholar 

  60. Henderson G, Cox F, Ganesh S, Jonker A, Young W, Global Rumen Census Collaborators, et al. Rumen microbial community composition varies with diet and host, but a core microbiome is found across a wide geographical range. Sci Rep. 2015;5:14567.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  61. Nollet L, Demeyer D, Verstraete W. Effect of 2-bromoethanesulfonic acid and Peptostreptococcus productus ATCC 35244 addition on stimulation of reductive acetogenesis in the ruminal ecosystem by selective inhibition of methanogenesis. Appl Environ Microbiol. 1997;63(1):194–200.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  62. Duin EC, Wagner T, Shima S, Prakash D, Cronin B, Yáñez-Ruiz DR, et al. Mode of action uncovered for the specific reduction of methane emissions from ruminants by the small molecule 3-nitrooxypropanol. Proc Natl Acad Sci U S A. 2016;113(22):6172–7.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  63. Patra A, Park T, Kim M, Yu Z. Rumen methanogens and mitigation of methane emission by anti-methanogenic compounds and substances. J Anim Sci Biotechnol. 2017;8:13.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  64. Thauer RK. Methyl (alkyl)-coenzyme M reductases: nickel F-430-containing enzymes involved in anaerobic methane formation and in anaerobic oxidation of methane or of short chain alkanes. Biochemistry. 2019;58(52):5198–220.

    Article  CAS  PubMed  Google Scholar 

  65. Abbott DW, Aasen IM, Beauchemin KA, Grondahl F, Gruninger R, Hayes M, et al. Seaweed and seaweed bioactives for mitigation of enteric methane: challenges and opportunities. Animals. 2020;10(12):2432.

    Article  PubMed  PubMed Central  Google Scholar 

Download references


The authors wish to thank Isabel Jiménez, Rafael Núñez (SIC-EEZ) and Juan N. Moliz (CIC-UGR) for their assistance in the samples analyses.


This work was funded by Blue Ocean Barns. AB has a Ramón y Cajal research contract (RYC2019-027764-I) funded by the Spanish State Research Agency (AEI).

Author information

Authors and Affiliations



DRY, AB, JKS and EK designed the experiments. PR, EJ and RH performed the experiments. PR and AB analysed the experimental data. PR wrote the draft manuscript. DRY, AB, ER, JKS and EK reviewed and edited the manuscript. All authors read and approved the final version.

Corresponding authors

Correspondence to Alejandro Belanche or David R. Yáñez-Ruiz.

Ethics declarations

Ethics approval and consent to participate

Animal Care and Use Committee approval was not obtained for this study because there were no animal-handling practices; the rumen fluid used in the in vitro incubations was obtained after slaughtering of animals in a commercial slaughterhouse. The authors had no direct control over the care of the animals included in this study.

Consent for publication

Not applicable.

Competing interests

The authors declare that they have no competing interests.

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit The Creative Commons Public Domain Dedication waiver ( applies to the data made available in this article, unless otherwise stated in a credit line to the data.

Reprints and Permissions

About this article

Check for updates. Verify currency and authenticity via CrossMark

Cite this article

Romero, P., Belanche, A., Jiménez, E. et al. Rumen microbial degradation of bromoform from red seaweed (Asparagopsis taxiformis) and the impact on rumen fermentation and methanogenic archaea. J Animal Sci Biotechnol 14, 133 (2023).

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI: