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Temporal changes in microbial community composition during cultureenrichment experiments with Indonesian Coals
Rita Susilawati, Paul N. Evans, Joan S. Esterle, Steven J. Robbins, Gene W.Tyson, Suzanne D. Golding, Tennille E. Mares
PII: S0166-5162(14)00225-0DOI: doi: 10.1016/j.coal.2014.10.015Reference: COGEL 2394
To appear in: International Journal of Coal Geology
Received date: 24 July 2014Revised date: 30 October 2014Accepted date: 30 October 2014
Please cite this article as: Susilawati, Rita, Evans, Paul N., Esterle, Joan S., Robbins,Steven J., Tyson, Gene W., Golding, Suzanne D., Mares, Tennille E., Temporal changesin microbial community composition during culture enrichment experiments with Indone-sian Coals, International Journal of Coal Geology (2014), doi: 10.1016/j.coal.2014.10.015
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TITLE:
Temporal changes in microbial community composition during culture enrichment experiments
with Indonesian Coals
CONTRIBUTORS:
Rita Susilawatia,b,*, Paul N. Evansc, Joan S. Esterlea, Steven J. Robbinsc, Gene W. Tysonc, Suzanne D.
Goldinga, Tennille E. Maresa
AFFILIATIONS:
a School of Earth Sciences, The University of Queensland, St Lucia, Queensland 4072 Australia;
b Geological Agency of Indonesia, Jl. Sukarno Hatta no 444, Bandung, West Java 40254, Indonesia;
c Australian Centre for Ecogenomics, School of Chemistry and Molecular Biosciences,
The University of Queensland, St Lucia, Queensland 4072, Australia.
*Corresponding author
ABSTRACT
Temporal changes in microbial community structures during methanogenesis were
investigated in cultures of South Sumatra Basin (SSB) coalbed methane (CBM) formation water
(SSB5) grown on three coals of different rank (Burung sub bituminous Rv 0.39%, Mangus sub
bituminous Rv 0.5%, Mangus anthracite Rv 2.2%). Methane production accelerated from day 6,
peaked around day 17 and then levelled off around day 20. The initial bacterial community from the
SSB formation water was predominantly Acetobacterium, Acidaminobacter, Bacteriodes and
Pelobacter species, while the archaeal community consisted of Methanosaeta, Methanosarcina and
Methanobacterium members. A general pattern was observed in all cultures with the three coals.
Over time the bacterial members decreased in proportion whereas the archaeal component
increased. The increase in the proportion of archaeal methanogens corresponded with an increase
in methane production yield.
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Enrichment cultures produced similar communities when grown on coals from the same
seam (Mangus sub bituminous and Mangus anthracite), rather than from different seams of similar
type (Burung sub bituminous and Mangus sub bituminous). Methanosaeta was the dominant
methanogen species in the sub bituminous Burung coal culture, but was a lesser proportion in
cultures of both Mangus sub bituminous and anthracite coals where Methanosarcina species were a
greater proportion. Interestingly, obligate hydrogenotrophic methanogens from the genera of
Methanobacterium, which were present at low levels in culture enrichment of all coal substrates,
increased in proportion only in the absence of coal in the no-coal control enrichment cultures. These
results suggest that the low rank Burung sub bituminous coal favours methane production by the
obligate acetoclastic Methanosaeta members while both Mangus coals also favour metabolically
versatile Methanosarcina members, and the absence of coal favours hydrogenotrophic
methanogens. Despite the similarity of communities grown on coals from the same seam, greater
quantities of methane were generated from the lower rank coals when compared to higher rank
coals.
Keywords: coal; microbial community; methanogenesis; coal bed methane
1. Introduction
Once considered to be an unconventional energy source, coal bed methane (CBM) has
become a significant energy resource in many countries (Moore, 2012; Strąpod et al., 2011). Over
the last decade, the focus of CBM research has shifted from identifying and extracting the resource
to replenishing the methane by stimulating the native microbial community to form methane in situ
by degrading the deep coal, effectively turning coal seams into real-time methane bioreactors. The
potential for coal as a methane-forming bioreactor has been assessed in several coal basins
worldwide (Fry et al., 2009; Green et al., 2008; Guo et al., 2012; McIntosh et al., 2008; Papendick et
al., 2011; Penner et al., 2010; Singh et al., 2012; Strąpod et al., 2008)
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Methane in coal seams can be produced as a by-product of the thermal coalification process
(thermogenic) and by methanogenic activity (biogenic). Isotope analysis of the methane extracted
from some CBM reservoirs has revealed biogenic origins, and have speculated that real time
methane could be formed from the in situ coal in those reservoirs (Butland and Moore, 2008; Faiz
and Hendry, 2006; Flores et al., 2008; Golding et al., 2013; Hamilton et al., 2014; Kinnon et al., 2010;
Mares and Moore, 2008; Strąpod et al., 2007; Susilawati et al., 2013). To this end, several laboratory
based studies of the culture-dependant and independent methods have shown the presence of
active microbial consortia able to form methane from coal in a number of CBM reservoirs (Guo et al.,
2012; McIntosh et al., 2008; Papendick et al., 2011; Penner et al., 2010; Singh et al., 2012; Strąpod et
al., 2008). These results suggest the potential exists to develop new and renewable biogenic gas
resources from deep coal seams.
Despite microorganisms being present in coal and its associated formation waters, the
ability of the microbial community to deconstruct the coal is still poorly understood due to the
heterogeneously complex physical and chemical structure of the coal and to the limited number of
studies that identify coal degrading microbial species (Faison, 1991; Fakoussa and Hofrichter, 1999;
Strąpod et al., 2011). Consequently, the mechanism in which the microbial consortium degrades the
complex organic substrate into methane from coal remains unknown. A limited number of studies
have shown coal degradation begins with hydrolysis of polyaromatic, aromatic and other
hydrocarbon substrates into compounds such as volatile fatty acids (VFAs), alcohols and other
organic acids, which in turn are formed into methanogenic substrates such as acetate,
hydrogen/carbon dioxide and methanol (Jones et al., 2010; Strąpod et al., 2011). Bacterial species
from the genera Bacteroides, Pelobacter, Clostridium and Spirochaetes detected in coal and
associated formation waters have been implicated in hydrolysis of hydrocarbons (Aklujkar et al.,
2012; Kudo et al., 1987; Murray, 1986; Sträuber et al., 2012). However, despite being implicated in
hydrocarbon degradation from CBM wells, those bacterial species are often found to be fermenters
upon closer examination (Wawrik et al., 2014). In CBM reservoirs, those bacteria are typically found
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associated with hydrogenotrophic (e.g. Methanobacterium and Methanocorpusculum spp.),
acetoclastic (e.g. Methanosaeta and Methanosarcina spp.) and methylotrophic methanogens (e.g.
Methanolobus spp.) (Doerfert et al., 2009; Ghosh et al., 2014; Green et al., 2008; Midgley et al.,
2010; Penner et al., 2010; Singh et al., 2012; Strąpod et al., 2008; Tang et al., 2012).
Although broad similarities in the structure of the microbial consortia exist, each CBM
reservoir site has a unique community structure that differs with respect to its primary community
members and their dominance. Despite the broad understanding of the communities, only a few
studies have reported the influence of differing coal substrates on methane production from native
coalbed microbial communities (Fallgren et al., 2013a; Jones et al., 2008; Susilawati et al., 2013). To
this end, we investigated the microbial communities present in a previously unstudied South
Sumatra Basin (SSB) CBM reservoir and the temporal changes in its microbial community structure
during growth on three native SSB coals of different rank.
2. Geology of the South Sumatra Basin
The geology of the SSB has been outlined by de Coster (1974), Darman and Sidi (2000) and
Bishop (2001). The widespread accumulation of peat was transformed into the coals of the SSB
during the regressive phase of the Neogene depositional cycle (de Coster, 1974). A major regressive
sequence of Late Miocene-Pliocene sediments were deposited as the Barisan mountains uplifted
resulting in the deposition of the Muara Enim Formation, the main coal bearing unit in the SSB
(Koesoemadinata, 2000). During the deposition of the Muara Enim Formation, the tectonic setting of
the SSB produced a laterally extensive coal in respect of thickness, mineral matter and split pattern,
caused by exceptionally consistent subsidence coupled with the right type of climate (Stalder, 1976).
Coalification in the Muara Enim Formation on a regional scale was controlled predominantly by
burial depth variations as the geothermal gradient was relatively constant throughout the basin
(Stalder, 1976). The higher gradient encountered in some areas results from the localised effects of
igneous intrusions (Amijaya and Littke, 2006; Moore et al., 2014; Susilawati and Ward, 2006).
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Coal of the Muara Enim Formation has been exploited for decades at the Bukit Assam field,
where the three main coal seams (Mangus, Suban and Petai) have an average aggregate thickness
from 30 to 40 m. Several minor seams (eg. Benuang and Burung), lenticular shales, sandstones,
carbonaceous mudstones, and tuffaceous marker horizons are interbedded within these coals
(Figure 1).
3. Indonesian CBM
Indonesia is only just beginning to develop its CBM resources, and the SSB has been
highlighted as the most promising CBM basin in Indonesia (Figure 1), estimated to hold around 183
Tcf of CBM resources (Stevens and Hadiyanto, 2004). The coal in the SSB ranges from in depth 300-
1000 m and is mostly sub bituminous (Rv 0.4-0.5%) in rank with high vitrinite contents (> 90%) and
extremely low ash yields (< 5%). Most Indonesian low rank coals are composed of hydrogen rich
organic components (Davis et al., 2007) that are thought to make them excellent substrates for
biogenic methane generation.
To date, only two studies have reported the potential for biogenic CBM in Indonesia coal
basins. Gas isotopic analysis and preliminary enrichment work by Susilawati et al. (2013) identified a
biogenic origin for CBM in the SSB, and highlighted the potential of its coal and formation water for
future natural gas regeneration. Additionally Fallgren et al. (2013b), demonstrated methane
production from an Indonesia South Sumatra lignite and formation water for which there is no
previous history of gas production. To date, no study has reported the microbial methanogen
community structure in SSB CBM reservoirs.
3. Materials and methods
3.1. Coal sampling and analysis
Collection of coal directly from producing CBM reservoirs was unfortunately not possible, at
such, coal was sampled in May 2012 at PT Bukit Asam, a nearby coal mine in Tanjung Enim SSB.
Three Bukit Asam coals representing different coal seams; Burung sub-bituminous (Burung SB),
Mangus sub-bituminous (Mangus SB) and Mangus anthracite (Mangus A) were used in this study
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(Figure 1, Table 1). The rank of the two Mangus coals differed due to the effects of an igneous
intrusion into the coal seam. Coal samples were collected from the inner side of a fresh mining face
after digging out about 10 cm of surface coal to minimize the chance of samples being oxidised.
After coal lithotype description, fresh samples were wrapped with aluminium foil and plastic film,
placed in a box and stored at 4oC for one week before being shipped to Australia for culture
enrichment purposes. In the laboratory, coal samples were stored in an anaerobic chamber, to
avoid further oxidation processes. Time from collection to anaerobic chamber storage was less than
2 weeks.
The outer layer of the coal was pared away before the coal was crushed in the anaerobic
chamber using a mortar and pestle, milled using an electric coffee grinder and sieved to collect the
220 to 350 μm fractions. Subsequent petrographic analysis did not show any identifiable oxidation.
The crushed coal was then split into two parts using a riffle splitter, for chemical-physical analysis,
and for enrichment studies (used as sole carbon and energy substrate). ALS Laboratory, Queensland,
conducted coal chemical analyses (proximate and ultimate) while coal physical analyses (rank and
petrographic composition) were conducted using a Polarised Light microscope Leica DM4500 P LED
at the School of Earth Sciences, the University of Queensland, and Australia.
3.2. Formation water collection
Formation water for microbial culturing was collected anoxically from a CBM pilot
production well SSB5, located approximately 300 km south of Palembang, South Sumatra, Indonesia,
in May 2012. The formation water came from a depth of 609 m where the SSB5 well intersects the
Mangus seam. The formation water was flushed for one minute through a Norprene® rubber tube
connected to the SSB5 well water line before the water was collected into multiple 1L Mason jars by
overflowing the jar twice and sealing to exclude air. The Mason jars had been previously autoclaved
and flushed with nitrogen gas and filled with 1 ml reduction solution which consisted of 3 g sodium
sulphide nonahydrate, 0.675 g sodium hydroxide, 2.69g L-cysteine hydrochloride and 20 µL resazurin
dissolved in 30 ml of anoxic deionized water. The formation water samples were imported to
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Australia following Australian Quarantine and Inspection Service (AQIS) guidelines under permit no
IP13002699. In the laboratory, the formation water was stored in an anaerobic chamber (COY
laboratory Products, MI, USA) with an atmosphere of 95% nitrogen and 5% hydrogen.
A water sample from the SSB5 pilot well was also collected for anion and cation
concentration analysis. The analysis was conducted at the Centre of Groundwater Resource and
Environmental Geology in Bandung, Indonesia.
3.3. Enrichment culture experimental conditions
Experiments were designed to assess community changes during the process of biogenic
methane formation in culture enrichments of SSB5 formation water as inoculant and three SSB coals
as carbon substrates. Basal coal-based medium, as described in Papendick et al. (2011) and
Susilawati et al. (2013), was used for the microbial enrichment culture work and was prepared under
anoxic conditions according to the methods outlined by these authors.
Culture tubes were prepared in 26 mL tubes (Bellco Glass) where 0.25 g of coal substrate
(<300 μm) was combined with 9 mL of basal medium and capped with a butyl rubber stopper and
then removed from the chamber. Outside the chamber, using the gasing manifold and syringe, the
headspace was vacuumed and flushed with nitrogen 3 times to remove oxygen, then pressurized to
5 psig with nitrogen before being autoclaved at 121oC for 15 min. Culture tubes without added coal
(no-coal controls) were prepared as negative controls to test the ability of the microbial community
to form methane from coal. Other tubes with both coal and 20 mM 2-bromoethanesulfonic acid
(BESA) were also prepared as abiotic controls. Inside an anaerobic chamber and using a sterile 21-
gauge syringe needle, 3 mL of formation water was transferred into autoclaved culture tubes as the
inoculum. Before inoculation, filter-sterilized vitamin solution (Tanner, 2002) was injected into all
tubes (0.1 mL/ tube) using a 1 mL sterile syringe. Cultures were then incubated at 37oC until they
reached the stationary phase where cumulative methane concentrations no longer increased.
As previous experiments using the SSB5 formation water revealed that the growth of the
culture is in the range of 20-25 days (data not reported), eight replicate tubes for each coal
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enrichment culture were prepared to capture the different growth phases (lag, log, peak and
stationary). Changes in the relative abundance of the microbial communities during growth on each
of the coal enrichment cultures were assessed using a molecular analysis method. For this purpose,
one tube that produced the second highest methane yield from each set of coal enrichment cultures
was terminated every 2-3 days starting at day six. Terminated cultures were transferred into sterile
15 ml falcon tubes and centrifuged at 3270 × g for 30 min. The supernatant was discarded, and the
pellet frozen at -20°C until required for DNA extraction.
3.4. Measurement of Enrichment Culture Parameters and statistical analyses
Methane measurement was conducted every 2-3 days on all replicates tubes for each
culture to generate methane production profiles. Headspace gas was drawn from culture tubes
using an aseptic, anoxic technique. Headspace gas was drawn from the tubes using a Hamilton 1710
gas tight syringe and manually injected into a Varian 9700 Gas Chromatograph equipped with a 1177
column and a flame ionization detector (FID). Methane was calibrated using a 1%, 4% and 10% CH4
standard (Scientific and Technical Gases Ltd, UK).
Statistically significant differences of means in all culture treatments were evaluated by
two–way analysis of variance (ANOVA) and post hoc multiple comparison t-tests using Holm-Sidak
method, with alpha = 5.000% (Graph Pad Prism 6). For multiple comparison tests, each row was
analysed individually, without assuming a consistent standard deviation (SD). The means of methane
production and standard deviation at each time point (lag, log, peak, stationary) were calculated and
plotted as bar charts using Graph Pad Prism 6 (Graph Pad Software, Inc).
3.5. Growth curve and microbial community analysis
For the terminated enrichment culture tubes, the four that corresponded to the lag, log,
peak and stationary phases were selected for DNA extraction and community profiling. For
comparison, microbial community analysis was also performed on initial formation water (day 0) and
no-coal control cultures (day 10 and 20). DNA was extracted from the frozen enrichment culture cell
pellets using the phenol:chloroform:isoamyl alcohol method of Robbins et al. (in preparation) that
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was developed specifically for coal extractions. For community profiling, approximately 20 ng of
extracted DNA from enrichment cultures was used as a template for polymerase chain reaction PCR.
The 16S rRNA gene was PCR amplified using the universal primers 926F and 1392R under the
reaction conditions described in (Mondav and Woodcroft et al., 2014). Amplicons were sequenced
on the Roche 454 GS-FLX Titanium platform at the Australian Centre for Ecogenomics, University of
Queensland, Australia.
The resulting sequence reads were demultiplexed and chimeric sequences removed using
the UCHIME software (Edgar et al., 2011), while homopolymer errors were corrected using Acacia
(Bragg et al., 2012). Using QIIME scripts sequences were clustered into operational taxonomic units
(OTUs) at a 97% cut-off. A representative sequence was then randomly selected within each cluster
which is then given a taxonomic affiliation by performing a BLASTN search against the Greengenes
16S rRNA gene database (DeSantis et al., 2006). The results in the form of the abundance of
different OTUs and their taxonomic assignments in each sample are tabulated. To avoid misleading
statistical comparisons that could results from different sequencing depths and comparisons of
diversity with the bias of uneven sampling effort (a higher number of low-abundance OTUs will be
recovered by chance with increasing sequencing effort), the number of reads was normalized to
1150, to match the sample with the lowest number of sequences. Measures of microbial diversity
(Shannon index), species community richness (Chao 1) and composition skew (Evenness) were
estimated using the program EstimateS.
4. Results
4.1. Water chemistry
The SSB5 formation water is sodium bicarbonate-chloride type, and has very low
concentration of sulphate and low concentration of calcium and magnesium (Table 1). These
signatures are typical of formation water associated with CBM (Papendick et al., 2011; Taulis and
Milke, 2007; Van Voast, 2003). The dissolution of carbonate minerals such as calcium carbonate and
magnesium carbonate may contribute to the calcium, magnesium and bicarbonate levels in the
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water. However, significantly high bicarbonate alkalinities of SSB5 water may also indicate that the
source of dissolved inorganic carbon is from other than carbonate dissolution. The same phenomena
was also noticed in the Forest City Basin (McIntosh et al., 2008). It has been suggested that a high
concentration of bicarbonate in the water indicates the microbial decomposition of reduced carbon
stored in organic matter. The SSB5 water has higher total dissolved solid as shown by higher
concentration of sodium and chloride. Sulphate in SSB5 water was only detected in very low
concentration and that may not favour the growth of bacterial sulphate reducers.
4.2. Coal characterisation
Petrographic analysis (Table 2) showed that the Burung SB coal was the lowest rank (Rv =
0.39%) followed by the Mangus SB (Rv = 0.5%) and the Mangus A (Rv = 2.2%). Huminite in Burung SB
and Mangus SB coals or vitrinite in Mangus A coal were the major maceral groups present in the
coals and accounted for 81-97% of maceral composition. Liptinite group content is 6-7%, and
inertinite group content varies from 2-12% (Table 2). All three coals had very low mineral matter (≤
1%; corroborated by low ash yields <10%), which is typical for Indonesian coal. The anthracite by
comparison had much lower moisture and higher reflectance and as a result, higher vitrinite content
as the liptinite group macerals were devolatilised.
4.2. Methane production from coal enrichment cultures
Negligible amounts of methane produced from BESA treated abiotic control tubes (data
were not presented) suggested that little methane in cultures was from methane adsorbed in the
substrate coal. Overall, methane from each of the enrichment cultures increased slowly until day 6.
After day 6, methane production increased significantly and continued until around day 17 when the
peak of methane yield was achieved (Figure 2). After day 10, methane production rate started to
decline and was confirmed by day 20 when no increases in methane were seen for all coal types and
no-coal controls (Figure 2).
Using two-factor Anova, the difference between the methane production yields from the
four culture treatments (three cultures with coal substrate and 1 control) over time was analysed.
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The Anova test produced P values less than 5% for the three parameters being measured
(interaction, row and column factor) (Table 3) suggesting that methane production in this
experiment was affected by both time and substrate. Although the mean and maximum methane
production in all coal cultures were higher than no coal control culture, post hoc multiple
comparison test showed that only the Burung cultures consistently showed statistically significant
differences in their methane concentration compared to the no-coal control cultures whereas no
significant differences were observed in the mean between both Mangus cultures and no-coal
control cultures (Table 4). At peak production (day 17), the methane produced by the Burung
cultures was also significantly higher than other coal treated cultures (Figure 2, Table 4). This result
suggests there is some ability of the SSB5 microbial community to metabolise the coal and indicates
the influence of coal substrate to methanogenesis in SSB5 cultures. Even though differences in
methane concentration among the 3 coal cultures were not all statistically significant according to
the ANOVA test, the mean of methane production data indicated declining methane production
yields with increased rank (Figure 2). Burung SB coal culture has the highest methane production
yield, followed by the Mangus SB and Mangus A coal as the least (Figure 2). However, the rank trend
observed in the maximum total production rate is not as evident in the net rate (treatment ─
control) (Figure 3).
It has been reported that headspace gas composition and media bicarbonate concentrations
can have a significant effect on gas and methane production in culturing experiments (Lin et al.,
2013; Patra and Yu, 2014). The concentration of bicarbonate in our media was shown to have no
deleterious effect on coal to methane rate and yields (Papendick et al., 2011). Bicarbonate in the
inoculum may provide excess CO2, which in the presence of H2 rich substrates may stimulate
methanogenesis. The headspace gas containing H2 can provide hydrogen needed by
hydrogenotrophic methanogens to reduce CO2 to produce methane (Patra and Yu, 2014). Although
we use H2N2 as a gas mix in our anaerobic vessel, the presence of this gas in our culture tubes was
replaced by N2, as such the influence of additional H2 to the methane production in our experiment
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can be eliminated. Nitrogen can be a limiting factor (in the hydrolysis phase) but also as a source for
fermentation for subsequent methane production by methanogenic archaea (Wagner et al., 2012).
We did not test the effect of N2 gas on our methane production. However, since all cultures,
including the no-coal control, were treated similarly with 125 kPa N2, the presence of this gas in our
culture headspace will not affect treatment comparisons.
4.3. Microbial community
4.3.1. Microbial diversity
At the 97% cut-off score for an operational taxonomic unit (OTU), a total of 46 bacterial and
10 archaeal genera were observed in the SSB5 microbial communities grown on the Burung SB,
Mangus SB and Mangus A coals. Those OTUs over 1% are shown in Tables 5 and 6. The microbial
community of the Burung SB enrichment cultures had both the highest bacterial and archaeal
diversities among the coal enrichment cultures (Table 7 and 8), and produced the greatest quantity
of methane (Figure 2). For all three coals rank enrichment cultures, the bacterial diversity and
community skew, measured by evenness, decreased. Archaeal diversity and skew remained static
across all time points (Table 7 and 8).
The SSB water bacterial sequences were dominated by members of the Pelobacter and
Acetobacterium genera across all cultures and time points, while other species belonging to the
orders Bacteriodetes, Spirochaetes, Synergistetes and Tenericutes were consistently present at low
levels (Table 5). For the archaeal component of the communities, all enrichment cultures were
dominated by acetoclastic methanogens from the genera of Methanosaeta (Figure 4 and Table 6).
Lower levels of Methanosarcina, Methanobacterium, Methanospirillum and Candidatus
Methanoregula were also detected across all enrichment cultures whereas members belonging to
Methanofollis, Methanomethylovorans and Thermoplasmata were only found at very low
abundance in most cultures (<1%) and are grouped in Table 6 as “other archaea”.
4.3.2. Temporal changes in community structure
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The initial formation water contained a community composed of 14% bacteria and 86%
archaea. Culturing successfully enriched the bacterial communities, and by day six (the beginning of
log phase), the relative abundance of bacteria had almost doubled. At day six, the bacterial
population was at its highest proportion in all three cultures (bacteria 43-48% and archaea 52-57%)
and the community structure was similar between all three cultures, owing to the same inoculum
source. Over time the relative abundance of the bacterial population tended to decline, dropping
from 43-48% at day 6 to 15-29% by day 20. In contrast, in the no-coal controls, during the log phase
(day 10) bacteria occupied 17%, but increased to 28% at stationary phase (day 20), whereas archaea
decreased from 83% at day 10 to 71% at day 20.
In the Burung SB culture, the proportion of Acetobacterium and Pelobacter were similar with
both tending to decrease with time, whereas in the Mangus SB, Mangus A and no-coal control
cultures, Pelobacter is more dominant than Acetobacterium. The Burung SB culture had the highest
Bacteriodales population. Molecular analysis showed significant variations in methanogen
communities, with shifts in the dominance of different groups (Figure 4). It appeared that in the
Burung SB culture, most of the methane production was associated with growth of the obligate
acetoclastic methanogen, Methanosaeta. At day six, in both Mangus SB and Mangus A, the
acetoclastic (Methanosaeta) and hydrogenotrophic methanogens (Methanoregula and
Methanospirllium) were present in almost the same proportion but then decreased toward the end
of growth. In contrast, despite its low proportion at the early stage of growth, Methanosarcina was
present in significant proportions at the stationary phase. In the no-coal control culture,
Methanosaeta was the dominant methanogen until day 10. However, at the end of experiment
Methanosarcina and Methanobacteria were found to be equivalent in abundance. The
Methanobacteriales population was only observed in the early growth stage of Burung SB culture
and at the late stage of no-coal control culture. Its closest match was to the Methanobacterium
formicicum type strain.
5. Discussion
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5.1. Methane production
Although the differences are not considered significant by the ANOVA tests, the total and
net methane production from the experiments increased consistently over time, with some variation
attributable to the rank of the coal substrates. The small differences between methane yield from
coal tubes and no-coal controls in our experiment was likely to be a result of low concentration of
critical coal degrading bacterial consortium in the initial formation water inoculum, as such only
small amount of coal organic material can be biodegraded. Moreover, during storage, it is likely that
a key nutrient needed for the rapid growth of the microbial community available in the initial
formation water becomes depleted, or toxic by-products of microbial metabolism were
accumulated, which further influenced the growth of microbial communities capable of converting
coal to methane. Additionally, it seems that many organic constituents are also available as
substrates in the initial formation water, likely from continued microbial metabolism. This product
along with fine coal particles carried over in the water can provide substrates for metabolism in coal
and no-coal enrichment cultures.
The variation in methane production amongst experimental coal and no-coal control
replicate tubes may relate to the concentration of microbial methanogen consortium member
present in each 3ml of the inoculum added to these experimental systems. Each tube likely
contained slightly varying concentrations of the critical microbial methanogen consortium member,
which then led to differences in the methane yield. It can be assumed that the tube with the highest
methane production contains the highest concentration of critical consortium members. The fact
that differences showed a consistent change with rank could be coincidental, or reflect the influence
of coal on the process.
Our data suggests that the source of carbon for methane production in all SSB5 cultures was
from both the additional coal substrate and the inoculum (Figure 3). The greatest influence of coal
substrate occurred from day 6 to 10. In general, total production rate was higher than net
production rate, indicating that the organic precursor in the inoculum was easier to biodegrade than
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the additional coal substrate. This is not surprising since the consortia may well have adapted to the
native source of carbon present in the water.
5.2. Microbial methanogen community structure
In the future, CBM resources may become an important energy supplement to meet some
of the global demand for energy resources. Replenishment of current and future CBM resources by
in situ methanogenesis is one way to increase the productive lifetime of these fields but is
dependent on the ability of coal to be degraded by microbial communities. To this end, we tested
the ability of Indonesian coals to provide substrates for a native microbial community from an
Indonesian CBM well. The results of our experiments suggest that these coals can provide carbon
and energy source for a microbial consortium. Lower rank coals produced slightly more methane
than the higher rank coal in the experiments. Whereas cultures grown on coals of similar rank and
type produced different community structures, coal of the same seam with different rank revealed
similarity in their community structures, suggesting that community structure could be dependent
on coal source.
After an initial lag phase, typical of lag phases observed by other researchers for microbial
consortia grown on coal (Green et al., 2008; Papendick et al., 2011), the microbial population was
consistent among all enrichments grown on coal and consisted predominantly of the obligate
acetoclastic Methanosaeta methanogen species. However, due to the time taken to start
enrichment experiments, it is likely that a key nutrient needed to drive the metabolism of the
microbial consortia might have forced the community to this structure. As little methane was
formed during the lag phase, the Methanosaeta members are potentially significant constituents of
the original formation water inoculum, which is consistent with other studies that show
Methanosaeta species as a large proportion of indigenous communities (Jones et al., 2010; Wawrik
et al., 2012). The predominant bacterial members of the community during this lag phase were
Acidaminobacter, Acetobacterium and Pelobacter. The members of these bacteria are known to be
able to hydrolize and ferment aromatic compounds and hydrocarbons (Kreikenbohm and Pfennig,
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1985; Schink, 2006a; Sträuber et al., 2012) and have previously been identified in studies of coal
associated enrichment cultures across several CBM reservoirs (Barnhart et al., 2013; Dawson et al.,
2012; Green et al., 2008; Jones et al., 2010; Penner et al., 2010; Strąpod et al., 2011; Wawrik et al.,
2012). It is likely these bacteria were the primary degraders of coal constituents in our cultures.
Moreover, the involvement of Acetobacterium in the utilization of substrates produced by coal
degradation has been suggested by Barnhart et al. (2013). Consistent with this result, our
experiment showed that Acetobacterium species were always lesser proportions of the no-coal
community over the time series compared to coal containing cultures, suggesting that
Acetobacterium species likely metabolise substrates directly from the coal, even though the exact
mechanisms remain unknown.
After the lag phase, methane production increased rapidly and reached maximum
production rate by day 11 in all enrichment cultures. During this time the relative proportions of the
microbial community measured at days 10 and 17 had changed from day 6, with an increased
archaeal and corresponding decreased bacterial fraction. This result suggested that methanogenesis
was occurring from hydrolysis and fermentation end products produced by the bacterial component.
As the proportion of the obligate acetoclastic Methanosaeta had increased, such as in the Burung
microcosm, it is likely that it syntrophically consumes the acetate being produced by the Pelobacter,
Acetobacterium and Acidaminobacter members, which are known acetogens (Beckmann et al., 2011;
Green et al., 2008; Schink, 1997; Schink, 2006a, b; Stams and Hansen, 1984; Stams, 1994). It has
been reported that acetate production can eventually inhibit the growth of Acetobacterium, but in
the presence of Methanosaeta, acetate is utilised to produce methane and carbon dioxide (Bainotti
et al., 1997; Winter and Knoll, 1989). Acetobacterium would likely compete with hydrogenotrophic
methanogens for hydrogen when grown on coal which may explain why the proportion of
hydrogenotrophic methanogens only increased in the no-coal controls culture in the near absence of
Acetobacterium. Based on the ability of Methanosaeta to outcompete Methanosarcina species for
acetate (Liu and Whitman, 2008), the dominance of the Methanosaeta members over
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Methanosarcina species suggests that in our experiment acetate was only present at low
concentrations. Furthermore, Methanosarcina members observed in our study were closely related
to Methanosarcina mazeii, a versatile strain that is able to metabolise H2-CO2, acetate,
methylamines and methanol (Hovey et al., 2005; Jäger et al., 2009), therefore an increase in the
proportion of Methanosarcina species likely accounted for increases in methane concentration and
could be due to these members being able to metabolise methylated compounds such as
methylamines, methyl sulphide and methanol when produced towards the end of fermentation
(Allison and Macfarlane, 1989).
During the times between 10 and 17 days it became apparent that the communities on the
different coals diverged. The microbial community grown with the Mangus SB coal was more similar
to the Mangus A coal, than to the Burung SB coal. Pelobacter species were more dominant in both
Mangus cultures than in Burung SB culture. In the Mangus coal communities, Methanosarcina
became a significant proportion while in the Burung enrichment it was present in low proportion.
The increase of Methanosarcina in both Mangus cultures is concomitant with the decrease of both
Methanosaeta and Methanoregula. We postulated that both Mangus coals substrates reduced the
particular contribution of the obligate acetoclastic methanogen Methanosaeta and the obligate
hydrogenotrophic methanogen Methanoregula to methane production. On the contrary both coal
substrates increased the relative contribution of Methanosarcina to methane production in the
cultures. Methanosarcina has versatile methanogenic pathways, thus depending on the
environment condition these microbes may have advantage to produce methane via an effective
pathway and outcompete the other methanogen genera. In the end, it appeared that Burung coals
led to the growth of Methanosaeta while both of the Mangus coals stimulated the growth of
Methanosarcina. Except that the coals come from the same seam, it is not clear what factors are
responsible for the similarities in the microbial communities of cultures on Mangus SB and A coals.
The two coals have different chemical and petrographic properties due to the significant differences
in rank, but formerly shared the same origin and may have some characteristics that force the
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communities to reach a similar population structure. Although the communities on the Mangus SB
was similar to Mangus A coals, maximum methane produced from the Mangus SB was higher than
Mangus A, suggesting that the coal rank has an effect in the ability of the community to generate
methane. Overall, there also appeared to be an inverse correlation between maximum methane
yield and coal rank which is in agreement with previous studies (Scott, 1999; Strąpod et al., 2011).
The lower rank coal Burung SB culture is likely to be less recalcitrant and is easier to be biodegraded
than higher rank Mangus anthracite coal. It has been reported that an increasing recalcitrant
material has an inhibitory effect on methanogenesis (Minderlein and Blodau, 2010). It is likely that
the coal maturity and the organofacies of the source material govern the dominant extractable
compounds and their concentrations in the coal samples (Glombitza et al., 2009).
By day 20, methane production had ceased, and differences between the methane
concentrations of the microbial consortia when grown on the three coal substrates were still
observed when compared to the no coal control, although these differences were not always
significant. Interestingly, in the no-coal control enrichment cultures, the proportion of the
acetoclastic Methanosaeta species decreased significantly whereas the proportion of the obligate
hydrogenotrophic methanogens Methanobacterium increased which suggested that
hydrogen/carbon dioxide and not acetate are more important intermediates in microbial
metabolism in cultures without a coal substrate. Overtime we noted that in all cultures there was a
tendency that the bacterial members decreased in proportion whereas the archaeal component
increased and the increase in methanogen population corresponded with an increase in methane
production yield (Figure 5)
6. Conclusion
In this study, we show that an Indonesian CBM well produced an active methane-forming
microbial community, which adds to the known basins where microbial communities can form
methane from coal. The diversity of the community derived from the Indonesian coal formation
water was similar to previous studies that have enriched for microbial communities from coal basins
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worldwide. Further, to enrichment culture study and microbial community profiling, we show
community structure changes over time, which exhibited more similarity when grown on coal from
the same seam but of different ranks (Mangus SB and Mangus A), than to coal from similar rank
(Mangus SB and Burung SB). It is noteworthy that the enrichment culture grown on the lowest rank
coal produced the greatest quantity of methane, whereas the highest rank coal produced the least
methane per gram of coal. Overall, our results indicate a potential relationship between coal type,
microbial community composition and methane production. Further work should focus on factors
that may enhance or limit coal methanogenesis. We also highlight the need for more detailed
studies on coals of different type and ranks and their potential for microbes to form methane.
7. Acknowledgment
Australian Awards Scholarship provided funding for this research. The TSOP Spackman
award was used to fund part of laboratory consumables and gas isotope analyses for this study. PT
Medco CBM Sekayu and PT Bukit Asam kindly allowed site and sample access. The authors thank
Gordon Southam for constructive review of this manuscript, also Soleh Basuki Rahmat, Eko Budi
Tjahyono and Erlina Lena Ria from Geological Agency of Indonesia for field assistance.
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Figure Captions
Fig.1. Location of the study area: a) Water sampling (SSB5 well: blue dot) and coal sampling (black
dot); b) Coal stratigraphy of Bukit Asam area. Coal samples used in this study are from Burung and
Mangus seams. Stratigraphy of the coal seam is modified from Amijaya and Littke (2006).
Fig.2. Plot of average methane production from Burung (Brg), Mangus Sub Bituminous (MSb),
Mangus Anthracite (Ma) and No coal-control (Ncc) cultures. Error bars represent standard deviation
for replicates tubes.
Fig.3. Maximum methane production rate in SSB5 cultures, plotted as total rate (rate from
treatment tube where source of carbon came from both coal substrate and native fine coal particle
or dissolved constituent present in inoculum) and net rate (rate from treatment tubes subtracted by
no-coal control where coal is a major carbon substrate).
Fig.4. Bar charts depicting microbial methanogen community dynamics and diversity at phylum level
in SSB5 cultures during different stages of growth; a) Burung, b) Mangus Sub bituminous, c) Mangus
Anthracite, d) Inoculum (initial formation water at time 0 and no-coal controls at day 10 and 20).
Microbial communities presented in the graphs are the ones that occupy at least 1% of the total
microbial community in any stage of growth. Bacterial community displayed as area with solid colour
while methanogen community displayed as area with pattern.
Fig.5. Cross plot of methanogen abundance against methane yield in SSB5 cultures. Level of
confidence (P = 0.05) plot as dot line.
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Table Captions
Table 1. Formation water properties.
Table 2. Petrographic and chemical composition of coal samples used in this study. Bases are as
determined (a.d.b) and dry ash free (d.a.f).
Table 3. Analysis of Variance (ANOVA) results of methane productions in SSB5 culture experiments
Table 4. Post Hoc multiple comparison test of methane production in SSB5 culture experiments
Table 5. The dominant bacterial taxa detected in SSB5 cultures and the closest matches at 99%
similarity to known bacteria in GeneBank database.
Table 6. The dominant archaeal taxa detected in SSB5 cultures and the closest matches at 99%
similarity to known bacteria in GeneBank database.
Table 7. Bacterial diversity in SSB5 cultures during different stages of growth.
Table 8. Archaeal diversity in SSB5 cultures during different stages of growth.
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Fig 1a
Fig 1.b
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Fig 2
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Fig 3
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6 10 17 20
Mic
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Time (days)
Burung (Rv 0.39)
Proteobacteria
Spirochaetes
Firmicutes
Bacteriodetes
Methanosarcinae
Methanosaetaceae
Methanospirillaceae
Methanoregulaceae
Methanobacteriaceae
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Time (days)
Mangus (Rv 0.5)
Proteobacteria
Spirochaetes
Firmicutes
Bacteriodetes
Methanosarcinae
Methanosaetaceae
Methanospirillaceae
b)
a)
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Fig.4.
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Mangus (Rv 2.2) Proteobacteria
Spirochaetes
Firmicutes
Bacteriodetes
Methanosarcinae
Methanosaetaceae
Methanospirillaceae
Methanoregulaceae
Methanobacteriaceae
c)
0
20
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60
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100
0 10 20
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Time (days)
Formation water and no-coal control Proteobacteria
Spirochaetes
Firmicutes
Bacteriodetes
Synergistales
Methanosarcinae
Methanosaetaceae
Methanospirillaceae
Methanoregulaceae
Methanobacteriaceae
d)
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Fig. 5
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Table 1.
SSB5 water parameters Concentration
Temperature 32
pH 6.63
Salinity(ppm) 1350
Conductivity(mS) 3.3
CO32- (mg/L) nd
HCO3- (mg/L) 942.5
SO42-(mg/L) 3
Cl- (mg/L) 439.5
Ca2+ (mg/L) 9.7
Mg2+ (mg/L) 6.2
Na+ (mg/L) 577.9
K+ (mg/L) 126.1
Trace elements
Cu (mg/L) 0.025
Zn (mg/L) 0.318
Ni (mg/L) nd
Co (mg/L) 2.97
Pb (mg/L) 0
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Tabel 2
Analysis Burung Sb Mangus Sb Mangus A
Proximate % (a.d.b)
Moisture 16.8 8 1.2 Ash 2.2 0.7 1.2 Volatile matter 38.1 42.5 14.7 Fixed carbon 42.9 48.8 82.9 Total sulphur 0.83 0.34 1.06
Ultimate % (d.a.f)
Carbon 76.2 78.2 91 Hydrogen 5.14 5.26 3.83 Nitrogen 1.67 1.15 1.56 Sulphur 1.02 0.37 1.09 Oxygen (By difference) 15.9 15.1 2.6
Petrography (%)
Rv (Rank) 0.39 0.5 2.2 Maceral composition
Huminite/Vitrinite
Textinite 6 3
Ulminite 23 22
Attrinite 24 20
Densinite 17 27
Corpohuminite 8 4
Gelinite 4 5
Total 82 81 97 Inertinite
Fusinite 5 3
Semifusinite 1 1
Funginite 2 5
Inertodetrinite 2 3 2 Macrinite 0 0
Total 10 12 2 Liptinite
Sporinite 1 1
Cutinite 1 1
Resinite 1 0
Liptodetrinite 2 2
Suberinite 1 2
Exsudatinite 1 0 0 Total 7 6 0 Mineral matter 1 1 1
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Table 3
ANOVA table SS DF MS F (DFn, DFd) P value
Interaction 1315 9 146.1 F (9, 62) = 2.414 P = 0.0203
Time 46199 3 15400 F (3, 62) = 254.4 P < 0.0001
Treatments 5659 3 1886 F (3, 62) = 31.16 P < 0.0001
Residual 3753 62 60.53 SS=sum of square, DF= degree of freedom, MS= mean of square, DFn= degrees of freedom numerator, Dfd= degrees of freedom denominator. DFn= a-1, DFd= N-a, a=number of treatments, N= the total number of measurement.
Table 4
Time (days)
Post hoc multiple comparison test (Holm Sidak method)
Brg vs MSb
Brg vs MA
Brg vs Ncc
MSB vs MA
MSB vs Ncc
MA vs Ncc
MSB vs Ncc
MA vs Ncc
6 < 0.001 < 0.001 < 0.001 0.150 0.370 0.630 0.370 0.630
10 0.020 0.240 0.001 0.600 0.039 0.080 0.039 0.080
17 0.006 0.005 0.002 0.400 0.037 0.181 0.037 0.181
20 0.024 0.010 0.012 0.347 0.088 0.402 0.088 0.402 Brg= Burung, MSb= Mangus Sub-bituminous, Ma= Mangus Anthracite, Ncc= no-coal control
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Table 5.
No Closest BLAST Sequence match Origin of closest match Affinity
1
Bacteroidetes bacterium AY548787
Metal-Containing Wastewater
Bacteria; Bacteroidetes; Bacteroidia; Bacteroidales; unclassified_Bacteroidales
2
Geovibrio ferrireducens X95744
Surface sediment of hydrocarbon-contaminated ditch
Bacteria; Deferribacteres; Deferribacterales; Deferribacteraceae; Geovibrio.
3
Acetobacterium carbinolicum AB546236 Oil storage tank
Bacteria; Firmicutes; Clostridia; Clostridiales; Eubacteriaceae;Acetobacterium.
4
Acidaminobacter hydrogenoformans AF016691 Black mud
Bacteria; Firmicutes; Clostridia; Clostridiales; Clostridiales Family XII. Incertae Sedis; Acidaminobacter.
5
Azospira sp. R-25019 AM084030
Municipal wastewater treatment plant
Bacteria; Proteobacteria; Betaproteobacteria; Rhodocyclales; Rhodocyclaceae; Azospira
6
Uncultured bacterium GQ181535
Purified terephthalic acid (PTA) wastewater
Bacteria; Proteobacteria; Deltaproteobacteria; Desulfovibrionales;Desulfovibrionaceae; Desulvofibrio.
7
Desulfomicrobium sp AY570692
Production water of oil reservoir
Bacteria; Proteobacteria; Deltaproteobacteria; Desulfovibrionales; Desulfomicrobiaceae; Desulfomicrobium.
8
Uncultured bacterium AB701661 Natural gas field
Bacteria; Proteobacteria; Deltaproteobacteria; Desulfuromonadales; Pelobacteraceae; Pelobacter
9
Geobacter pelophilus U96918
Freshwater enrichment culture
Bacteria; Proteobacteria; Deltaproteobacteria; Desulfuromonadales; Geobacteraceae; Geobacter.
10
Uncultured bacterium GQ181438
Purified terephthalic acid (PTA) wastewater
Bacteria; Spirochaetes; Spirochaetales; Spirochaetaceae; Treponema.
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Table 6.
No Closest BLAST Sequence match Origin of closest match Taxonomic String
1
Methanobacterium formicicum AF169245
Culture collection, Institute of Microbiology CAS China
Archaea; Euryarchaeota; Methanobacteria; Methanobacteriales; Methanobacteriaceae; Methanobacterium
2
Uncultured Methanospirillaceae archaeon S000591267 river sediment
Archaea; Euryarchaeota; Methanomicrobia; Methanomicrobiales; Methanospirillaceae; Methanospirillum.
3
Methanoregula formicica AB479390 granular sludge
Archaea; Euryarchaeota; Methanomicrobia; Methanomicrobiales; Methanomicrobiales_incertae_sedis; Methanoregula.
4
Uncultured archaeon JN397698 River bank sediment
Archaea; Euryarchaeota; Methanomicrobia; Methanosarcinales; Methanosaetaceae; Methanosaeta.
5
Methanosarcina mazeii DQ987528
Isolated strain from Lake sediment
Archaea; Euryarchaeota; Methanomicrobia; Methanosarcinales; Methanosarcinaceae; Methanosarcina
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Table 7.
Inoculum (Raw Formation
water and No-Coal control)
Burung Sub-bituminous
Mangus Sub-bituminous
Mangus Anthracite
Micobial Taxa RFW C10 C20 6 10 17 20 6 10 17 20 6 10 17 20
Bacteriodetes
o_Bacteriodales 3.2 1.6 0.4 0.9 0.6 0.3 0.8 0.7 0.7 0.9 1 0.7 0.5 0.4 0.4
Firmicutes
Acidaminobacter 0.0 0.2 0.0 1.4 0.6 0.1 0.0 1.9 1.0 0.0 0.1 2.1 1.0 1.0 2.4
Acetobacterium 2.7 6 0.1 19.6 6.4 4.1 5.0 11.8 4.2 4.1 6.7 14.1 8.2 6.3 7.7
Proteobacteria
f_Comamonadaceae 0.3 0.1 0 0 0.1 0.1 0.2 0.1 0.0 2.3 0 0.1 0.1 0.1 0
Desulfomicrobium 0.0 0.1 0 0.1 0.0 0.1 0.0 0.2 0.0 1.2 0.2 0.0 0.4 0.6 0.1
Desulfovibrio 0.0 0.5 0.4 0.5 0.9 0.3 0.7 0.6 0.2 1.0 0.7 0.3 0.5 0.3 0.5
f_Geobacteraceae 0.0 0.0 0.0 0.0 0.0 0.0 0.0 0.0 0.2 1.7 0.0 0.0 0.0 0.0 0.0
f_Pelobacteraceae 2.4 5.3 23.3 16.9 6.0 3.9 5.1 29.1 11.7 25.7 15.9 30.0 22.8 21.2 12.6
Spirochaetes
Treponema 0.6 0.2 1.0 0.7 0.4 0.7 1.5 0.6 0.3 0.2 0.9 0.3 0.5 0.9 0.3
All Synergistetes 1.4 0.3 0.8 0.3 0.1 0.2 0.2 0.5 0.3 0.0 0.7 0.2 0.4 0.3 0.1
All Tenericutes 1.0 0.3 0.0 0.0 0.0 0.2 0.2 0.0 0.0 0.0 0.0 0.0 0.1 0.0 0.1
Other Bacteria 2.8 2.7 2.3 2.8 1.0 1.5 1.6 0.8 0.8 2.1 2.3 0.4 2.0 1.5 0.7
Total read abundance of Bacteria Taxa (% of normalized OTU read)
14.4 17.3 28.3 43.2 16.1 11.5 15.3 46.3 19.4 39.2 28.5 48.2 36.5 32.6 24.9
Species richness (Chao 1) 33.9 22.5 20.5 33.1 14.5 18.48 21.1 34.9 35.9 19.9 18.9 38.9 21.5 15.0 23.9
(24. 5, (20.4, (18.4, (27.1, (13.2, (16.4, (19.3, (20.9, (26.7, (15.8, (14.7, (23.1, (15.3, (15.67, (21.5,
75.9) 35.2) 34.9) 58.3) 28.0) 32.9) 32.3) 98.1) 78.1) 47.1) 46.0) 104.2) 56.4) 16.2) 38.9)
Evenness 0.8 0.7 0.4 0.5 0.6 0.7 0.7 0.4 0.5 0.5 0.5 0.4 0.5 0.5 0.5
Shannon Diversity Index
2.4
(0.08)
2.0 (0.07)
1.0 (0.03)
1.5 (0.03)
1.6 (0.04)
1.8 (0.08)
1.9 (0.09)
1.1 (0.02)
1.4 (0.04)
1.3 (0.02)
1.4 (0.06)
1.2 (0.02)
1.4 (0.04)
1..4 (0.02)
1.6 (0.04)
OTU= Operational Taxonomy Unit; RFW =Raw Formation Water; C10 = control at day 10, C20 = control at day 20. p= phylum, c= class, o= ordo, f=family.
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Evenness calculated as H/ln(S), H=Shannon Diversity, S= Chao 1. For Chao 1, values between brackets represent lower bound and upper bound.
For Shannon Diversity Index, values between brackets are standard deviation. Only taxa that has read abundance ≥1% from total are plotted in this table.
Taxa that has read abundance <1% was grouped together. Dominant taxa are highlighted
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Table 8.
Inoculum
(Raw Formation water and No-Coal Control)
Burung Sub-bituminous
Mangus Sub-bituminous
Mangus Anthracite
Micobial Taxa RFW C10 C20 6 10 17 20 6 10 17 20 6 10 17 20
Methanobacteriales
Methanobacterium 0.1 0.0 36.6 9.3 0.0 0.1 0.1 0.2 0.0 0.0 0.1 0.2 0.0 0.0 0.2
Methanomicrobiales
Candidatus Methanoregula 23.5 9.0 0.0 12.3 11.7 7.8 7.2 17.9 14.6 8.4 11.3 21.1 6.8 7.8 9.8
Methanospirillum 8.9 2.4 0.0 2.0 3.7 3.1 1.5 4.3 4.2 8.4 3.2 4.5 2.6 1.3 3.2
Methanosarcinales
Methanosaeta 50.7 65 16.4 26.4 61.2 70.8 71.1 29.2 48.1 43.6 22.9 21.1 38.7 33.8 26
Methanosarcina 1.3 6.0 18.2 6.7 7.0 5.9 4.3 1.8 13.6 0.5 33.6 4.2 14.9 24.4 35.3
Other archaea 1.4 0.3 0 0.5 0.6 0.8 0.6 0.8 0.1 0.2 0.6 1.1 0.7 0.3 0.5
Total read abundance of Archaea Taxa (% of normalised OTU read)
85.9 82.7 71.2 57.2 84.2 88.5 84.8 54.2 80.6 61.1 71.7 52.2 63.7 67.6 75.0
Species richness (Chao 1) 8.0 7.0 7.0 8.0 10.5 7.0 11.0 8.0 8.0 11.0 7.0 8.0 6.0 6.0 7.0
(8.0, (7.0, (6.1, (8.2, (9.2, (7.0, (8.4, (8.0, (8.4, (8.4, (7.0, (8.1, (6.0, (6.1, (7.1,
8.9) 8.0) 19.7) 9.1) 24.1) 8.1) 32.9) 9.4) 9.1) 32.9) 8.4) 9.1) 7.4) 7.2) 8.1)
Evenness
0.5
0.4
0.6
0.7
0.4
0.4
0.3
0.6
0.5
0.5
0.6
0.5
0.6
0.5
0.6
Shannon Diversity Index 1.1 (0.00)
0.8 (0.00)
1.1 (0.00)
1.4 (0.01)
0.9 (0.00)
0.7 (0.00)
0.6 (0.00)
1.3 (0.01)
1.1 (0.00)
1.1 (0.00)
1.2 (0.00)
1.1 (0.01)
1.1 (0.01)
0.8 (0.00)
1.2 (0.02)
OTU= Operational Taxonomy Unit; RFW =Raw Formation Water; C10 = control at day 10, C20 = control at day 20. p= phylum, c= class, o= order, f=family.
Evenness calculated as H/ln(S), H=Shannon Diversity, S= Chao 1. For Chao 1, values between brackets represent lower bound and upper bound.
For Shannon Diversity Index, values between brackets are standard deviation. Only taxa that has read abundance ≥1% from total are plotted in this table.
Taxa that has read abundance <1% was grouped together. Dominant taxa are highlighted.
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Highlights
An active methane-forming microbial community presence in Indonesia CBM reservoir
Microbial community structure changed over time during growth and exhibited more
similarity when grown on coal from the same seam but of different ranks, than to coal from
similar rank and type.
The increase in methanogen population corresponded with an increase in methane
production yield.
The results of this study indicate a potential relationship between coal type and rank,
microbial community composition and methane production.