Next Article in Journal
“Everyone Has the Right to Drink Beer”: A Stakeholder Analysis of Challenges to Youth Alcohol Harm-Reduction Policies in Lebanon
Previous Article in Journal
Comparison of Short-Term Associations between PM2.5 Components and Mortality across Six Major Cities in South Korea
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
IJERPH
Volume 16
Issue 16
10.3390/ijerph16162873
ijerph-logo
Submit to this Journal Review for this Journal Propose a Special Issue
► Article Menu

Article Menu

share Share announcement Help format_quote Cite question_answer Discuss in SciProfiles thumb_up
...
Endorse textsms
...
Comment
first_page
settings
Order Article Reprints
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Article

Anaerobic Dechlorination by a Humin-Dependent Pentachlorophenol-Dechlorinating Consortium under Autotrophic Conditions Induced by Homoacetogenesis

by
Mahasweta Laskar
1,
Takanori Awata
2,
Takuya Kasai
1,3 and
Arata Katayama
1,3,*
1
Graduate School of Engineering, Nagoya University, Nagoya 464-8603, Japan
2
National Institute for Land and Infrastructure Management, Tsukuba 305-0804, Japan
3
Institute of Materials and Systems for Sustainability, Nagoya University, Nagoya 464-8603, Japan
*
Author to whom correspondence should be addressed.
Int. J. Environ. Res. Public Health 2019, 16(16), 2873; https://doi.org/10.3390/ijerph16162873
Submission received: 21 July 2019 / Revised: 3 August 2019 / Accepted: 9 August 2019 / Published: 11 August 2019
(This article belongs to the Section Environmental Science and Engineering)
Browse Figures
Versions Notes

Abstract

:
Anoxic aquifers suffer from energy limitations due to the unavailability of organic substrates, as dictated by hydrogen (H2) for various electron-accepting processes. This deficiency often results in the accumulation of persistent organic pollutants, where bioremediation using organic compounds often leads to secondary contamination. This study involves the reductive dechlorination of pentachlorophenol (PCP) by dechlorinators that do not use H2 directly, but rather through a reduced state of humin—a solid-phase humic substance—as the extracellular electron donor, which requires an organic donor such as formate, lactate, etc. This shortcoming was addressed by the development of an anaerobic mixed culture that was capable of reductively dechlorinating PCP using humin under autotrophic conditions induced by homoacetogenesis. Here, H2 was used for carbon-dioxide fixation to acetate; the acetate produced was used for the reduction of humin; and consequently used for dechlorination through reduced humin. The 16SrRNA gene sequencing analysis showed Dehalobacter and Dehalobacterium as the possible dechlorinators, while Clostridium and Oxobacter were identified as the homoacetogens. Thus, this work contributes to the development of an anaerobic consortium that balanced H2 dependency, where efficiency of humin reduction extends the applicability of anaerobic microbial remediation in aquifers through autotrophy, syntrophy, and reductive dechlorination.

1. Introduction

Aquifer contamination by persistent organic pollutants (POPs) is a matter of serious concern considering biogeochemical and atmospheric processes as drivers for the magnification of this issue to a global scale, impacting water, soil, and also the food chain [1,2,3,4]. The anoxic niche in aquifers harbors different types of microorganisms in an intertwined network, mainly dependent on hydrogen (H2) as the donor for different electron-accepting processes (e.g., NO3−, Mn(IV), Fe(III), SO42−, CO2) for their growth and metabolism. These H2-utilizing microbial reactions in turn make anaerobic bioremediation—especially anaerobic dehalogenation—a panacea for aquifer contamination removal [5,6]. Dehalococcoides is one such H2-utilizing dehalogenating microorganism (organohalide respirer) that has been found and characterized [7].
Pentachlorophenol (PCP), a POP currently listed under Stockholm Convention because of its carcinogenic and toxic effects, has received a great deal of attention as early as the 1970s, especially from its use as a pesticide in agricultural and wood preservation sectors [8,9,10]. In the anaerobic bioremediation or natural attenuation of PCP, reductive dechlorination is carried out by dechlorinators, where the chlorine atoms are substituted with hydrogen atoms (electrons) [11]. However, low growth or bioenergetics by such microorganisms is reflected by the high redox potential (+399 mV at pH 7 for PCP/2,3,4,5-tetrachlorophenol using H2); substrate, and nutrient limitation; and even geological composition [12,13]. For such bioenergetics metabolism, humic substances in soil help in crossing the energy barrier by transfer of electrons between the microorganisms and the electron-accepting compounds [14,15].
The catalytic centers present in soil for extracellular electron transfer (EET) have been explored in studies using humin, the insoluble humic substance in soil at any pH, which behaves as a redox mediator in reductive PCP dechlorination by the transfer of electrons from formate-oxidizing bacteria to the dechlorinators [16]. The humin-dependent dechlorinators did not use H2 as the electron donor, but required a reduced humin through input of an organic electron donor such as formate, or via electrochemically reduced humin [17,18,19]. The requirement of an organic electron donor has also been observed in other microbial reactions using humin, such as debromination of tetrabromobisphenol-A [20]; iron reduction, nitrate reduction to ammonia [18]; and denitrification [21].
It is already known that the introduction of organic electron donors has secondary impacts on bioremediation, such as excessive biomass growth, fouling, etc., and this concern has been addressed by the dissolution of H2 gas in aquifers for bioremediation [22,23]. We previously demonstrated that co-culturing the denitrifying bacterium Pseudomonas stutzeri JCM20778 with the acetogenic bacterium Sporomusa ovata DSMZ 2662 ensured denitrification in the absence of organic substrate by the use of the inorganic compounds H2 and carbon dioxide for substrate production [24]. Acetogenic microorganisms (e.g., Sporomusa ovata, Clostridium ljungdahlii, Moorella thermoacetica, etc.) utilize H2 for the production of organic acids such as acetate and oxobutyrate from CO2 in a process known as homoacetogenesis [25,26]. This suggests the manifestation of a hydrogenotrophic bioremediation system in coexistence with other microorganisms in an environment where carbon dioxide is indigenously present. The application of this phenomenon to organohalide-contaminated aquifers bioremediation is both lucrative and challenging, owing to the varying H2 requirement, as well as the redox potential (−290 mV from CO2/acetate) between dechlorinators and acetogens [27,28]. Concerning on humin-dependent PCP reductive dechlorination, the effect of autotrophy has not been observed until now. In this study, we developed a humin-dependent PCP-dechlorinating consortium with acetogenic activity, and demonstrated PCP reductive dechlorination through acetate oxidation that was produced due to homoacetogenesis using the inorganic compounds H2 and carbon dioxide.

2. Materials and Methods

2.1. Humin

Humin was prepared by a modified extraction method of the previous paper [16]. Air-dried Kamajima soil (600 g) was sieved with 2 mm mesh sieves. The sieved soil was mixed with 150 mL distilled water in a 250 mL centrifugation bottle and shaken by a mechanical shaker (Taitec TS-20, Tokyo, Japan) for 30 min. The bottle was kept upright for 7 s, and decantation was carried out in 30 s to remove larger mineral particles in the soil. The remaining soil was mixed and decanted again with 150 mL of distilled water in the same manner. The two-times decanted soil fractions were combined and subjected to the humin extraction procedure, consisting of a series of washings with mechanical shaking for 24 h with chemicals, as follows: twice with 150 mL of 0.1 N NaOH, four times with 2% HF; twice with 75 mL of 0.1 N NaOH, twice with 2% HF; and a final wash of four times with 0.1 N NaOH. The obtained humin was then washed twice with distilled water for 12 h. The obtained humin was neutralized at pH 7.0 ± 0.2 using 0.1 N HCl. The neutralized humin was then washed twice with distilled water with 12 h mechanical shaking. In all the washing steps, the centrifugation was carried out at 8000× g (Kubota 7780, Tokyo, Japan) for 15 min at 23 °C to separate humin as precipitate in the washing solutions. The obtained humin was freeze dried, ground finely using ceramic mortar, and subjected to the experiment.

2.2. Humin-Dependent PCP-Dechlorinating Culture (HMBC Culture)

The HMBC culture was obtained using 10 mM acetate as the sole electron donor and carbon source, with 1 g of humin inoculation of a PCP-dechlorinating culture grown on Kamajima soil using lactate as the electron donor and carbon source, which had been maintained in the laboratory [29]. The total 120 mL volume capacity of a serum glass bottle was filled with 50 mL of an anaerobic medium and sparged with a mixed gas ratio of 4:1 N2 and CO2 until pH 7.2 ± 0.2 was achieved. The bottle was capped with a Teflon-coated butyl rubber stopper and sealed with aluminum crimp. The headspace was flushed with mixed gas of N2 and CO2 (4:1) through an air filter with pores of 0.22 µm diameter for 30 min to expel remaining traces of oxygen. The culture was incubated at 30 °C in the dark for two weeks and transferred serially by 10-fold dilutions for maintenance until use. The medium consisted of: NH4Cl 1.0 g/L; CaCl2·2H2O 0.05 g/L; MgCl2·6H2O 0.1 g/L; K2HPO4 0.4 g/L; NaHCO3 4.0 g/L; CH3COONa 0.82 g/L; 1 mL of selenite-tungstate solution; 1 mL of trace elements solution SL-10 [30]; and 1 mL of resazurin (0.1 g in 100 mL pure water). Figure S1 shows the community structure of the HMBC culture.

2.3. Homoacetogenic Culture (HC Culture)

A HC culture had been maintained in the laboratory using a mineral medium by serial transfer of 5% (v/v) of the culture every 14 days of incubation. The mineral medium composition used was modified DSMZ 311a medium as follows: K2HPO4 0.35 g/L; KH2PO4 0.23 g/L; NH4Cl 0.5 g/L; MgSO4·7H2O 0.5 g/L; CaCl2·2H2O 0.25 g/L; NaCl 2.25 g/L; FeSO4·7H2O 0.002g/L; Yeast extract 0.1 g/L; NaHCO3 4 g/L; 1 mL of Selenite-Tungstate solution; and 1 mL of Trace Elements Solution SL-10. The mineral medium was sparged by the mixed gas of N2:CO2 until pH neutrality, and the headspace was flushed with H2 and CO2 (4:1) for 40 min post inoculation. Figure S2 shows the community structure of the HC culture.

2.4. Humin-Dependent PCP-Dechlorinating Culture with Acetogenic Activity (M-CO Culture)

The M-CO culture was obtained by mixing the HMBC and HC cultures in the ratio of 2:1. The M-CO culture was maintained in a mineral medium by serial transfer of 10% (v/v) of the culture. The mineral medium composition (Medium Z) consisted of: K2HPO4 0.4 g/L; NH4Cl 0.5 g/L; MgSO4. 7H2O 0.3 g/L; CaCl2·2H2O 0.15 g/L; NaCl 1.0 g/L; FeSO4·7H2O 0.002 g/L; NaHCO3 4.0 g/L; 1 mL of selenite-tungstate solution; 1 mL of trace elements solution SL-10; and 1 mL of resazurin (0.1 g in 100 mL pure water). The medium was sparged with a mixed gas ratio of 4:1 N2 and CO2 until pH 7.2 ± 0.2 was achieved. Vitamin solution [20], 20 µM sodium pentachlorophenol (>90% purity, Fujifilm Wako Pure Chemical Corporation, Osaka, Japan), and Ti-NTA solution (0.20 mM) were added prior to the inoculation. The headspace was flushed with H2 and CO2 (4:1) post inoculation.
The sterilization of the anaerobic medium for culture bottles HMBC, HC, and M-CO was carried out by steam sterilization at 121 °C for 20 min prior to the inoculation. The inorganic chemicals used in the study used Special Grade (JIS) chemicals, and were purchased from FUJIFILM Wako Pure Chemical Corporation, Osaka, Japan.

2.5. Effect of Conditions on the PCP Dechlorination in the Mixed Consortium M-CO

Effects of inoculation and humin were examined using the M-CO culture. The effect of sulfide was examined by adding Na2S into the M-CO-B culture, where 0.3 g/L of MgSO4. 7H2O in medium Z was replaced with MgCl2 6H2O of the corresponding concentration (medium ZN). Sulfate and salinity effects were examined in the HMBC culture by spiking with 0.5 g/L Na2SO4 and 2.25 g/L NaCl, respectively. Effects of humin oxidation and H2 were examined in the M-CO-B culture. The experimental conditions are summarized in Table 1.

2.6. Oxidized Humin Preparation

The oxidation of humin was carried out electrochemically using twisted platinum electrodes as working and counter electrodes (0.8 mm in diameter and 1 m in length), and a Ag/AgCl as reference electrode (+263 mV vs. SHE (Standard Hydrogen Electrode), Fusheng Analytical Instrument Co., Shanghai, China). The redox potential of 4 g humin in 150 mL anaerobic medium was maintained at 0 mV vs. Ag/AgCl electrode for 18 h. The oxidized humin was filtered using filter paper No. 2 (Advantec, Tokyo, Japan), and >0.9 g (approx.) oxidized humin was transferred to the respective triplicate cultures studied. The oxidation, filtration, and transfer of humin to the culture bottles was carried out in a vinyl anaerobic chamber (Coy-7450000, COY, Grass Lake, MI, USA).

2.7. Chemical and Headspace Analyses

PCP and metabolites were extracted and analyzed as described previously [29] using a GCMS QP2010 (Shimadzu, Kyoto, Japan) equipped with a DB-5ms column (J7W Scientific, Folsom, CA, USA). Chlorophenols with >90% purity (FUJIFILM Wako Pure Chemical Corporation, Osaka, Japan) were used as standards. Organic acids were analyzed by HPLC (Shimadzu LC-10AT, Kyoto, Japan) with a Puresil C18 reversed-phase column (Waters, Milford, MA, US) and a UV detector at 210 nm. The mobile phase was 0.1% H3PO4 which was previously filtered using 0.45-µm PTFE membrane (Omnipore™, Merck, Darmstadt, Germany). The samples were provided by filtering the culture using a 0.2-µm membrane (Omnipore™, Merck, Darmstadt, Germany). Glacial acetic and formic acids with >99% purity (Cica KANTO CHEMICAL CO., INC., Tokyo, Japan) and 50% sodium lactate solution (FUJIFILM Wako Pure Chemical Corporation, Osaka, Japan) were used as standards. H2, CO2, and CH4 in the headspace were measured by a GC-14B gas chromatograph equipped with thermal conductivity and flame ionization detectors (Shimadzu, Kyoto, Japan). Sampling was carried out using a 100 µL-volume pressure-lock PTFE syringe (VICI, Baton Rouge, LA, USA) using nitrogen as the carrier gas.

2.8. Microbial Community Structure

Microbial biomass was collected from the fifth generation, and the microbial DNA was extracted using a FastDNA SPIN kit for soil (MP Biomedicals, Japan, Tokyo, Japan). PCR amplification of the bacterial 16S rRNA gene was performed with a primer set for amplification of the V3–V4 region as follows: Pro341F (5′-CCT ACG GGN BGC ASC AG-3′) and Pro805R (5′-GAC TAC NVG GGT ATC TAA TCC-3′) [31]. The reaction mixtures contained 12.5 µL of KAPA HiFi HotStart Ready mix (KAPA Biosystems, Wilmington, MA, USA), 2.5 µL of Pro341F and Pro805R primers (2 µM each), and 5 µL of template DNA (5 ng/µL). The PCR condition was as follows: initial activation at 94 °C for 30 s, followed by 10 cycles at 94 °C for 10 s, 60 °C for 30 s, 72 °C for 30 s, followed by 10 cycles at 94 °C for 10 s, 59 °C for 30 s, 72 °C for 30 s, followed by 10 cycles at 94 °C for 10 s, 58 °C for 30 s, 72 °C for 30 s, and final extension at 72 °C for 4 min. The PCR products were purified using the AMPure XP kit (Beckman Coulter Genomics Inc., Brea, CA, USA) according to the manufacturer’s instructions. The PCR products were confirmed using a 1% agarose gel. The concentration of purified DNA was determined using a QuantiFluor dsDNA System (Promega Corporation, Fitchburg, WI, USA). Purified DNA was sequenced using a Miseq platform with a Miseq reagent kit v3 (600 cycle, Illumina Inc., San Diego, CA, USA). A chimera check was performed for the base sequences of each read obtained from the analysis using USEARCH v6.1 [32]. Reads with more than 97% sequence similarity were classified into the same operational taxonomic unit (OTU), and OTU picking and cluster analysis were performed in QIIME 1.8 [33]. OTUs were identified using the Greengenes database (ver. 13_8) [34].

3. Results

3.1. Dechlorination of PCP by M-CO Culture

Figure 1 shows PCP’s reductive dechlorination by the M-CO culture under autotrophic conditions after two weeks of incubation. The most prominent metabolites were 3,5-dichlorphenol (3,5-DCP) and 3,4,5-trichlorophenol (3,4,5-TCP), followed by 2,3,4,5-tetrachlorophenol (2,3,4,5-TeCP), 3-chlorophenol (3-CP), and occasionally phenol. The M-CO culture used H2 as the sole electron donor, and HCO3−/CO2 was the only carbon source; where bicarbonate (HCO3−) was added as a buffer for the medium, and the headspace was flushed with a mixed gas composed of H2 and CO2 (4:1). The mixed microbial consortium in the M-CO culture was developed by mixing the humin-dependent PCP-dechlorinating HMBC culture with the homoacetogenic CO2-fixing HC culture in the ratio of 2:1. Figure 2 shows the homoacetogenic activity observed in the M-CO culture. The acetate amount detected at Day 0 was a result of carry over by 10% (v/v) culture transfer, while acetate corresponding to Day 14 showed an increase from Day 0. The acetate production after two weeks of incubation agreed with the corresponding decrease of H2 and CO2 in the headspace, as shown in Figure 3. Methane generation was also observed in the headspace after two weeks of incubation. As PCP dechlorination was not observed in absence of the inoculum (basal condition) (Figure S3), PCP dechlorination under autotrophic condition was recognized due to microbial activity. Dechlorination activity was not observed in the cultures without humin (namely, the CO and HC-PCP cultures) (Figure S3), which indicated the dependency of this mixed consortium on humin for dechlorination activity. Note also that the dechlorination inactivity in the CO culture occurred despite external H2 addition, and acetate at a concentration larger than 1 mM present initially as carry over due to culture transfer. This suggested that the dechlorinating consortium here was unlike the typical organohalide respirers such as Dehalobacter restrictus or Dehalococcoides, which directly utilize H2 as electron donor and acetate as carbon source [35].

3.2. Inhibitory Factors in the M-CO Culture

The M-CO culture showed less dechlorinated metabolites in comparison to the metabolites observed for the parent dechlorinating HMBC culture (namely, 3-CP and phenol) (Figure S4), suggesting inhibitory effects. The blackish precipitation for the M-CO culture (Figure S5) indicated ferrous sulfide precipitation, where the sulfate concentration of 1.21 mM as sulfate in the medium Z exceeded the critical concentration of 100 µM producing the precipitation [14]. To examine the inhibitory effect due to sulfate reduction, the M-CO-B culture was provided in the medium ZN, where MgSO4·7H2O in medium Z was replaced with MgCl2·6H2O. Figure 4 shows the higher PCP dechlorination rate under autotrophic conditions in the M-CO-B culture than in the M-CO culture. The dechlorination metabolites for M-CO-B culture were 3-CP and phenol only. The effect of sulfide was further examined by adding 1.21 mM Na2S to the M-CO-B culture (i.e., MCO-Na2S culture). PCP dechlorination was not observed at all in the culture MCO-Na2S, indicating sulfide toxicity to be primarily the reason for the lower activity of the M-CO culture.
The inhibitory effects of sulfate and salinity were also tested for the parent dechlorinating HMBC culture. The dechlorinating culture contained 10 mM acetate as the electron donor, and H2 was not added externally. Addition of Na2SO4 to the HMBC culture (i.e., PCP-Sulfate culture) significantly inhibited PCP dechlorination, as shown by the lesser quantities of dechlorinated metabolites 2,3,4,5-TeCP, 3,4,5-TCP, 3,5-DCP, and 3-CP (Figure S6). Sodium chloride (NaCl) showed an even higher inhibitory effect for the HMBC culture (i.e., PCP-Sal culture) where 2,3,4,5-TeCP and 3,4,5-TCP (Figure S7) were the only observed metabolites. However, as NaCl was present for both medium Z and medium ZN, the inhibitory effect in the M-CO culture was not considered due to salinity, but sulfate reduction alone.

3.3. Role of Humin in Reductive Dechlorination

The role of humin was examined in the M-CO-B culture using oxidized humin at 0 mV (vs. the Ag/AgCl electrode) under conditions with and without the external addition of H2 to the headspace (i.e., the oxd-H2 and oxd-N2 cultures, respectively). Figure 5 shows higher dechlorination activity for the culture oxd-H2 than the culture oxd-N2, implying that externally added H2 acted as an electron donor for dechlorination by this mixed consortium. This was also supported by acetate detection (57.95 µmoles) only for the culture oxd-H2, but not for the culture oxd-N2. Lower, but still observed, dechlorination activity for the culture oxd-N2 was considered to be influenced by the carry-over acetate due to the inoculum transfer, as the theoretical requirement for complete dechlorination of 20 µM PCP is only 25 µM of acetate, as calculated from Equations (1) and (2) [36,37]:
2 C O 2 + 4 H 2 ↔ C H 3 C O O H ,
C 6 C l 5 O H + 5 H 2 → C 6 H 5 O H + 5 H C l .

3.4. Microbial Composition of M-CO Culture

Figure 6 shows the microbial community structure of the M-CO culture. The major microorganisms belonged to the phyla Euryarchaeota, Firmicutes, Proteobacteria, Bacteroidetes, and Chloroflexi. Euryarchaeota were mostly represented by the genus Methanobacterium, which utilize H2 and CO2 for methane production. The genera Methanoculleus and Methanomassiliicoccus were also detected as Euryarchaeota. Dehalobacter and Dehalobacterium were detected as the probable dechlorinating bacteria [35,37]. The acetate-producing activity from CO2 is characterized by the bifunctional and oxygen sensitive enzyme complex of carbon-monoxide dehydrogenase (CODH) and acetyl-CoA synthase (ACS) [38], which can be distributed into diverse groups: methanogenic archaea, and acetogenic bacteria including Firmicutes, Deltaproteobacteria, and Chloroflexi. Of these diverse groups, the microorganisms detected in the M-CO culture were clostridia: Clostridium and Oxobacter as the autotrophic acetogenic bacteria [39,40], and Caloramator as the possible heterotrophic acetogenic bacteria [41]. An OTU classified into Desulfovibrionaceae was identified as a potential sulfate reducer, and heterotrophic acetogen as well in the absence of sulfate [42,43]. Geobacter is known to have electroactive characteristics, is a utilizer of acetate as an electron donor [15], and was occasionally detected in the M-CO culture.
The Shannon diversity index [44] showed a diversity of 2.39 with an equitability of 0.24, emphasizing the richness of the phyla mentioned earlier. The Chao 1 Index [44] measured a total 85 OTUs for the observed 69 OTUs, which reflected approximately 24.08% influence by the minor microbial groups as influential.

4. Discussion

The microbial reductive dechlorination of PCP under autotrophic conditions was achieved by the cultures M-CO and M-CO-B, the mixed cultures obtained from the humin-dependent PCP-dechlorinating HMBC culture, and the homoacetogenic HC culture. The significant difference in the PCP dechlorination rate between the cultures with and without H2 (cultures oxd-H2 and oxd-N2, respectively) clearly demonstrated that H2 functioned as the electron donor for anaerobic dechlorination. No dechlorination was observed for the culture CO, confirming that dechlorinating organisms present in mixed culture did not utilize H2 as the electron donor, and that the presence of humin was essential as the external electron mediator for the dechlorinators. Additionally, acetate production in the cultures M-CO and M-CO-B was a result of homoacetogenesis. In a comparison between the cultures oxd-H2 and oxd-N2, acetate production was observed only for the culture oxd-H2, which accentuated the need of acetate as the secondary electron donor for humin reduction, and its consequent use for EET. These suggested that homoacetogenesis together with humin’s electron-mediating ability marked the pathway for syntrophic association to accommodate microbial reductive dechlorination under autotrophic conditions. A key syntrophic link between the acetogens, the acetate oxidizers involved in humin reduction, and the humin-oxidizing dechlorinators was established.
Table 2 shows the distribution of electrons from H2 used for different sinks (i.e., acetate production, methane generation, sulfate reduction, and PCP reductive dechlorination). The electron balance for the M-CO culture suggested that a significant portion of electrons from H2 were diverted towards methane generation and sulfate reduction. While electrons invested for acetate production were minimal, it was almost negligible for dechlorination. In comparison to the M-CO culture, the electron balance for the M-CO-B culture showed that the total H2 used exceeded the requirement of electrons spent for the respective sinks, demonstrating the presence of an unknown sink. The only plausible explanation for the unknown sink was humin, considering the characteristics of humin as a redox mediator under anaerobic conditions. This interpretation agrees with the electron balance showing a negative value in the culture oxd-N2, where PCP dechlorination was observed although no H2 was supplied as an electron donor. Here the negative value of electron balance showed the presence of an unknown electron donor for dechlorination and methane generation, most probably with humin acting as an electron donor. The addition of H2 (i.e., the culture oxd-H2) increased the PCP dechlorination rate, with a decreased dependency on the unknown electron donor, in addition to the production of acetate and methane. It should be also noted that although humin in the cultures of oxd-H2 and oxd-N2 was electrochemically oxidized at 0 mV vs. Ag/AgCl (i.e., +263 mV vs SHE) for 18 h, the oxidized humin was still active as an electron donor for PCP dechlorination and methane production. The redox center of humin as an electron mediator is considered difficult to be electrochemically oxidized.
The direct sinks of H2 (electron) were for acetogenesis, methanogenesis, and sulfate reduction, while PCP dechlorination was the indirect sink via the external electron transfer of humin. The threshold concentration of H2 is known to be higher in the order of acetogenesis (>0.7 meeq as electron), methanogenesis (0.01–0.2 meeq), and sulfate reducers (0.002–0.02 meeq) [27,49]. Therefore, the decrease of H2 distribution rate for acetogenesis would be unavoidable because of the predominance of methanogenesis and sulfate reduction, especially after the H2 concentration decreased. Sulfate reduction (sulfide production) resulted in an inhibitory effect on the PCP dechlorination, as well as reduced the electron flow for PCP dechlorination. The methanogens and sulfate-reducing microorganisms can use both acetate and H2 as electron donors in general [50]. However, in the M-CO culture, Methanobacterium was detected as the major methanogen and Desulfovibrionaceae as the major sulfate-reducing microorganism, and they are both hydrogenotrophic [43,51]. Therefore, the acetate produced would be mainly utilized for the humin reduction, although other acetate-utilizing reactions cannot be discarded. The microbial community analysis suggested Geobacter as the possible acetate-utilizing humin reducer. Humin oxidizers other than dechlorinators have not been identified. Further study should be carried out to determine the microorganisms involved in the reduction and oxidation of humin, which has potential as a versatile electron mediator for various microbial reactions [18].

5. Conclusions

An anaerobic mixed culture achieved 20 µM PCP reductive dechlorination in the absence of any form of external addition of organic substrates as carbon source or energy. An autotrophic environment dictated by homoacetogenesis resulted in the establishment of reductive PCP dechlorination by the cultures M-CO and M-CO-B. Electrons provided as H2 were utilized as direct sinks for acetate production, methane generation, and sulfate reduction. The acetate produced was used for humin reduction by the humin reducers (the indirect sink), and facilitated external electron transfer to the dechlorinators for PCP dechlorination. Humin thus worked as an interface between two specific groups—the humin-reducers and the humin-oxidizers—and thereby maintained a steady balance of electron diversion from acetate to be used for PCP dechlorination, as shown in Figure 7. The results extended the applicability of such a humin-dependent dechlorinating culture for bioremediation when supplied with only H2 as an electron donor, constraining secondary pollution in anoxic aquifers. However, sulfate limitations have to be properly understood in such cases, and the re-routing of electrons towards methanogenesis needs to be addressed, which results in overall decreased efficiency for such systems.

Supplementary Materials

The following are available online at https://www.mdpi.com/1660-4601/16/16/2873/s1. Figure S1: Microbial composition of the dechlorinating HMBC culture based on 16SrRNA gene sequencing. Figure S2: Microbial composition of the homoacetogenic HC culture based on 16SrRNA gene sequence. Figure S3: Remaining PCP after two weeks of incubation with no chlorophenol metabolites detected for the cultures under different conditions except for headspace containing H2:CO2 (1:4). Figure S4: PCP-dechlorinated phenolic metabolites detected in the HMBC culture after two weeks of incubation, where 10 mM acetate was used as organic electron donor and carbon source. Figure S5: Blackish precipitation observed in the M-CO culture (medium Z with headspace of H2 and CO2 (4:1)) after two weeks of incubation. Figure S6: Remaining PCP and chlorophenol metabolites detected in the HMBC culture after two weeks of incubation when spiked with 1.217 mM sulfate (PCP-Sulfate culture in Table 1). Figure S7: Remaining PCP and chlorophenol metabolites detected in the HMBC culture spiked with 2.25 g/L NaCl (PCP-Sal culture in Table 1) after two weeks of incubation. Table S1: Hydrogenolytic reactions using different electron acceptors that may occur for M-CO and M-CO-B cultures.

Author Contributions

Conceptualization, A.K.; Data Curation, M.L. and T.A.; Funding Acquisition, T.A., T.K., and A.K.; Methodology, M.L., T.A., T.K., and A.K.; Investigation, M.L.; Project Administration, A.K.; Writing—Original Draft Preparation, M.L.; Writing—Review and Editing, A.K.; Visualization, M.L.; Supervision, A.K.

Funding

This study was supported in part by a Grant-in-Aid for Scientific Research (17H01899) from the Japan Society for the Promotion of Science (JSPS), by cooperative study program of IMaSS, Nagoya University (2018 project), by JFE 21st Century Foundation (2019 project), and by the Institute for Fermentation, Osaka (L-2019-3-003).

Acknowledgments

The authors are immensely grateful to Toyoko Demachi and Shozo Ohta for their unceasing support in laboratory and technical assistance.

Conflicts of Interest

The authors declare no conflicts of interest. The funders had no role in the design of the study; in the collection, analyses, or interpretation of data; in the writing of the manuscript; or in the decision to publish the results.

References

  1. Bayen, S.; Wurl, O.; Karuppiah, S.; Sivasothi, N.; Hian, K.L.; Obbard, J.P. Persistent organic pollutants in mangrove food webs in Singapore. Chemosphere 2005, 61, 303–313. [Google Scholar] [CrossRef] [PubMed]
  2. Manz, M.; Wenzel, K.D.; Dietze, U.; Schüürmann, G. Persistent organic pollutants in agricultural soils of central Germany. Sci. Total Environ. 2001, 277, 187–198. [Google Scholar] [CrossRef]
  3. Weber, K.; Goerke, H. Persistent organic pollutants (POPs) in antarctic fish: Levels, patterns, changes. Chemosphere 2003, 53, 667–678. [Google Scholar] [CrossRef]
  4. Zhang, Z.L.; Hong, H.S.; Zhou, J.L.; Huang, J.; Yu, G. Fate and assessment of persistent organic pollutants in water and sediment from Minjiang River Estuary, Southeast China. Chemosphere 2003, 52, 1423–1430. [Google Scholar] [CrossRef]
  5. Holliger, C.; Gaspard, S.; Glod, G.; Heijman, C.; Schumacher, W.; Schwarzenbach, R.P.; Vazquez, F. Contaminated environments in the subsurface and bioremediation: Organic contaminants. FEMS Microbiol. Rev. 1997, 20, 517–523. [Google Scholar] [CrossRef]
  6. Lovley, D.R.; Chapelle, F.H. Deep subsurface microbial processes. Rev. Geophys. 1995, 33, 365–381. [Google Scholar] [CrossRef]
  7. Adrian, L.; Löffler, F.E. Organohalide-Respiring Bacteria; Springer: Berlin/Heidelberg, Germany, 2016; ISBN 978-3-662-49875-0. [Google Scholar]
  8. Nicholson, D.K.; Woods, S.L.; Istok, J.D.; Peek, D.C. Reductive Dechlorination of Chlorophenols by a Pentachlorophenol-Acclimated Methanogenic Consortium. Appl. Environ. Microbiol. 1992, 58, 2280–2286. [Google Scholar]
  9. Strycharz, S.M.; Gannon, S.M.; Boles, A.R.; Franks, A.E.; Nevin, K.P.; Lovley, D.R. Reductive dechlorination of 2-chlorophenol by Anaeromyxobacter dehalogenans with an electrode serving as the electron donor. Environ. Microbiol. Rep. 2010, 2, 289–294. [Google Scholar] [CrossRef]
  10. Watanabe, I. Pentachlorophenol (PCP) decomposing activity of field soils treated annually with PCP. Soil Biol. Biochem. 1978, 10, 71–75. [Google Scholar] [CrossRef]
  11. Holliger, C.; Schraa, G. Physiological meaning and potential for application of reductive dechlorination by anaerobic bacteria. FEMS Microbiol. Rev. 1994, 15, 297–305. [Google Scholar] [CrossRef]
  12. Dolfing, J.; Novak, I. The Gibbs free energy of formation of halogenated benzenes, benzoates and phenols and their potential role as electron acceptors in anaerobic environments. Biodegradation 2014, 26, 15–27. [Google Scholar] [CrossRef] [Green Version]
  13. Dercová, K.; Sejáková, Z.; Skokanová, M.; Barančíková, G.; Makovníková, J. Bioremediation of soil contaminated with pentachlorophenol (PCP) using humic acids bound on zeolite. Chemosphere 2007, 66, 783–790. [Google Scholar] [CrossRef]
  14. Schink, B. Microbially driven redox reactions in anoxic environments: Pathways, Energetics, and biochemical consequences. Eng. Life Sci. 2006, 6, 228–233. [Google Scholar] [CrossRef]
  15. Lovley, D.R. Microbial Fe(III) reduction in subsurface environments. FEMS Microbiol. Rev. 1997, 20, 305–313. [Google Scholar] [CrossRef]
  16. Zhang, C.; Katayama, A. Humin as an electron mediator for microbial reductive dehalogenation. Environ. Sci. Technol. 2012, 46, 6575–6583. [Google Scholar] [CrossRef]
  17. Zhang, D.; Zhang, C.; Li, Z.; Suzuki, D.; Komatsu, D.D.; Tsunogai, U.; Katayama, A. Electrochemical stimulation of microbial reductive dechlorination of pentachlorophenol using solid-state redox mediator (humin) immobilization. Bioresour. Technol. 2014, 164, 232–240. [Google Scholar] [CrossRef] [PubMed]
  18. Zhang, D.; Zhang, C.; Xiao, Z.; Suzuki, D.; Katayama, A. Humin as an electron donor for enhancement of multiple microbial reduction reactions with different redox potentials in a consortium. J. Biosci. Bioeng. 2015, 119, 188–194. [Google Scholar] [CrossRef]
  19. Zhang, C.; Zhang, D.; Xiao, Z.; Li, Z.; Suzuki, D.; Katayama, A. Characterization of humins from different natural sources and the effect on microbial reductive dechlorination of pentachlorophenol. Chemosphere 2015, 131, 110–116. [Google Scholar] [CrossRef]
  20. Zhang, C.; Li, Z.; Suzuki, D.; Ye, L.; Yoshida, N.; Katayama, A. A humin-dependent Dehalobacter species is involved in reductive debromination of tetrabromobisphenol A. Chemosphere 2013, 92, 1343–1348. [Google Scholar] [CrossRef]
  21. Xiao, Z.; Awata, T.; Zhang, D.; Zhang, C.; Li, Z.; Katayama, A. Enhanced denitrification of Pseudomonas stutzeri by a bioelectrochemical system assisted with solid-phase humin. J. Biosci. Bioeng. 2016, 122, 85–91. [Google Scholar] [CrossRef]
  22. Schnobrich, M.R.; Chaplin, B.P.; Semmens, M.J.; Novak, P.J. Stimulating hydrogenotrophic denitrification in simulated groundwater containing high dissolved oxygen and nitrate concentrations. Water Res. 2007, 41, 1869–1876. [Google Scholar] [CrossRef]
  23. Fang, Y.; Hozalski, R.M.; Clapp, L.W.; Novak, P.J.; Semmens, M.J. Passive dissolution of hydrogen gas into groundwater using hollow-fiber membranes. Water Res. 2002, 36, 3533–3542. [Google Scholar] [CrossRef]
  24. Xiao, Z.; Awata, T.; Zhang, D.; Katayama, A. Denitrification of Pseudomonas stutzeri coupled with CO2 reduction by Sporomusa ovata with hydrogen as electron donor assisted with solid-phase humin. J. Biosci. Bioeng. 2016, 122, 307–313. [Google Scholar] [CrossRef]
  25. Ragsdale, S.W.; Pierce, E. Acetogenesis and the Wood-Ljungdahl pathway of CO2 fixation. Biochim. Biophys. Acta Proteins Proteom. 2008, 1784, 1873–1898. [Google Scholar] [CrossRef]
  26. Nevin, K.P.; Hensley, S.A.; Franks, A.E.; Summers, Z.M.; Ou, J.; Woodard, T.L.; Snoeyenbos-West, O.L.; Lovley, D.R. Electrosynthesis of organic compounds from carbon dioxide is catalyzed by a diversity of acetogenic microorganisms. Appl. Environ. Microbiol. 2011, 77, 2882–2886. [Google Scholar] [CrossRef]
  27. Luijten, M.L.G.C.; Roelofsen, W.; Langenhoff, A.A.M.; Schraa, G.; Stams, A.J.M. Hydrogen threshold concentrations in pure cultures of halorespiring bacteria and at a site polluted with chlorinated ethenes. Environ. Microbiol. 2004, 6, 646–650. [Google Scholar] [CrossRef]
  28. Schuchmann, K.; Müller, V. Energetics and Application of Heterotrophy in Acetogenic Bacteria. Appl. Environ. Microbiol. 2016, 82, 4056–4069. [Google Scholar] [CrossRef] [Green Version]
  29. Yoshida, N.; Yoshida, Y.; Handa, Y.; Kim, H.K.; Ichihara, S.; Katayama, A. Polyphasic characterization of a PCP-to-phenol dechlorinating microbial community enriched from paddy soil. Sci. Total Environ. 2007, 381, 233–242. [Google Scholar] [CrossRef]
  30. Widdel, F.; Kohring, G.-W.; Mayer, F. Studies on Dissimilatory Sulfate-Reducing Bacteria that Decompose Fatty Acids III. Characterization of the Filamentous Gliding Desulfonemalimicolagen. nov. sp. nov. and Desulfonemamagnumsp. nov. Arch. Microbiol. 1983, 134, 286–294. [Google Scholar] [CrossRef]
  31. Takahashi, S.; Tomita, J.; Nishioka, K.; Hisada, T.; Nishijima, M. Development of a prokaryotic universal primer for simultaneous analysis of Bacteria and Archaea using next-generation sequencing. PLoS ONE 2014, 9, e105592. [Google Scholar] [CrossRef]
  32. Edgar, R.C. Search and clustering orders of magnitude faster than BLAST. Bioinformatics 2010, 26, 2460–2461. [Google Scholar] [CrossRef] [Green Version]
  33. Caporaso, J.G.; Kuczynski, J.; Stombaugh, J.; Bittinger, K.; Bushman, F.D.; Costello, E.K.; Fierer, N.; Peña, A.G.; Goodrich, J.K.; Gordon, J.I.; et al. QIIME allows analysis of high-throughput community sequencing data. Nat. Methods 2010, 7, 335–336. [Google Scholar] [CrossRef] [Green Version]
  34. McDonald, D.; Price, M.N.; Goodrich, J.; Nawrocki, E.P.; Desantis, T.Z.; Probst, A.; Andersen, G.L.; Knight, R.; Hugenholtz, P. An improved Greengenes taxonomy with explicit ranks for ecological and evolutionary analyses of bacteria and archaea. ISME J. 2012, 6, 610–618. [Google Scholar] [CrossRef]
  35. Elfantroussi, S.; Naveau, H.; Agathos, S.N. Anaerobic dechlorinating bacteria. Biotechnol. Prog. 1998, 14, 167–188. [Google Scholar] [CrossRef]
  36. Diekert, G.; Wohlfarth, G. Metabolism of homoacetogens. Antonie Van Leeuwenhoek 1994, 66, 209–221. [Google Scholar] [CrossRef]
  37. Holliger, C.; Wohlfarth, G.; Diekert, G. Reductive dechlorination in the energy metabolism of anaerobic bacteria. FEMS Microbiol. Rev. 1998, 22, 383–398. [Google Scholar] [CrossRef]
  38. Adam, P.S.; Borrel, G.; Gribaldo, S. Evolutionary history of carbon monoxide dehydrogenase/acetyl-CoA synthase, one of the oldest enzymatic complexes. Proc. Natl. Acad. Sci. USA 2018, 115, E1166–E1173. [Google Scholar] [CrossRef]
  39. Müller, V.; Frerichs, J. Acetogenic Bacteria. eLS 2013, 1–9. [Google Scholar] [CrossRef]
  40. Rainey, F.A. Oxobacter. In Bergey’s Manual of Systematics of Archaea and Bacteria (online); John Wiley & Sons, Ltd.: Chichester, UK, 2015; pp. 1–4. ISBN 9781118960608. [Google Scholar]
  41. Baena, S.; Patel, B.K.C. Caloramator. In Bergey’s Manual of Systematics of Archaea and Bacteria (online); John Wiley & Sons, Ltd.: Chichester, UK, 2015; pp. 1–10. ISBN 9781118960608. [Google Scholar]
  42. Esquivel-Elizondo, S.; Delgado, A.G.; Krajmalnik-Brown, R. Evolution of microbial communities growing with carbon monoxide, hydrogen, and carbon dioxide. FEMS Microbiol. Ecol. 2017, 93, 1–12. [Google Scholar] [CrossRef]
  43. Kuever, J. The family desulfovibrionaceae. In The Prokaryotes: Deltaproteobacteria and Epsilonproteobacteria; Rosenberg, E., DeLong, E.F., Lory, S., Stackebrandt, E., Thompson, F., Eds.; Springer: Berlin/Heidelberg, Germany, 2014; pp. 107–133. [Google Scholar]
  44. Kim, B.-R.; Shin, J.; Guevarra, R.B.; Lee, J.H.; Kim, D.W.; Seol, K.-H.; Lee, J.-H.; Kim, H.B.; Isaacson, R.E. Deciphering Diversity Indices for a Better Understanding of Microbial Communities. J. Microbiol. Biotechnol. 2017, 27, 2089–2093. [Google Scholar] [CrossRef] [Green Version]
  45. Battino, R. The Ostwald coefficient of gas solubility. Fluid Phase Equilibria 1984, 15, 231–240. [Google Scholar] [CrossRef]
  46. Ferry, J.G. CO Dehydrogenase of Methanogens. In Acetogenesis; Chapman and Hall Microbiology Series; Drake, H.I., Ed.; Springer: Boston, MA, USA, 1994; pp. 539–556. [Google Scholar]
  47. Oren, A. There Must be an Acetogen Somewhere. Front. Microbiol. 2012, 3, 2–3. [Google Scholar] [CrossRef]
  48. Ozuolmez, D.; Na, H.; Lever, M.A.; Kjeldsen, K.U.; Jørgensen, B.B.; Plugge, C.M. Methanogenic archaea and sulfate reducing bacteria co-cultured on acetate: Teamwork or coexistence? Front. Microbiol. 2015, 6, 1–12. [Google Scholar] [CrossRef]
  49. Cord-Ruwisch, R.; Seitz, H.-J.; Conrad, R. The capacity of hydrogenotrophic anaerobic bacteria to compete for traces of hydrogen depends on the redox potential of the terminal electron acceptor. Arch. Microbiol. 1988, 149, 350–357. [Google Scholar] [CrossRef]
  50. Madigan, M.T.; Martinko, J.M.; Bender, K.S.; Buckley, D.H.; Stahl, D.A. Brock Biology of Microorganisms, Global Edition: UEL, 15th ed.; Pearson Education Limited: Harlow, UK, 2015; ISBN 1292068310. [Google Scholar]
  51. Buan, N.R. Methanogens: Pushing the boundaries of biology. Emerg. Top. Life Sci. 2018, 2, 629–646. [Google Scholar] [CrossRef]
Ijerph 16 02873 g001 550
Figure 1. Remaining pentachlorophenol and the produced chlorophenols as the metabolites in the M-CO culture after two weeks of incubation. The values are the average of triplicate samples across three generations (nine bottles) with standard errors shown as vertical bars. 2,3,4,5-TeCP: 2,3,4,5-tetrachlorophenol; 3,4,5-TCP: 3,4,5-trichlorophenol; 3,5-DCP: 3,5-dichlorphenol; and 3-CP: 3-chlorophenol.
Figure 1. Remaining pentachlorophenol and the produced chlorophenols as the metabolites in the M-CO culture after two weeks of incubation. The values are the average of triplicate samples across three generations (nine bottles) with standard errors shown as vertical bars. 2,3,4,5-TeCP: 2,3,4,5-tetrachlorophenol; 3,4,5-TCP: 3,4,5-trichlorophenol; 3,5-DCP: 3,5-dichlorphenol; and 3-CP: 3-chlorophenol.
Ijerph 16 02873 g001
Ijerph 16 02873 g002 550
Figure 2. Increase of amount of acetate between Day 0 and Day 14 across three generations of the M-CO culture. The values are the average of the acetate amount measured for the respective triplicates of three generations (nine bottles), with standard errors shown as vertical bars.
Figure 2. Increase of amount of acetate between Day 0 and Day 14 across three generations of the M-CO culture. The values are the average of the acetate amount measured for the respective triplicates of three generations (nine bottles), with standard errors shown as vertical bars.
Ijerph 16 02873 g002
Ijerph 16 02873 g003 550
Figure 3. Changes in the composition of headspace gas between Day 0 and Day 14 for the M-CO culture. The bar graphs represent the average of triplicates across three generations (nine bottles), with standard errors shown as vertical bars.
Figure 3. Changes in the composition of headspace gas between Day 0 and Day 14 for the M-CO culture. The bar graphs represent the average of triplicates across three generations (nine bottles), with standard errors shown as vertical bars.
Ijerph 16 02873 g003
Ijerph 16 02873 g004 550
Figure 4. Dechlorination rate (%) in the M-CO and M-CO-B cultures after two weeks of incubation. The bar graphs represent the dechlorination rate calculated based on total organic chloride dechlorinated between Day 0 and Day 14 of incubation as a measure of dechlorination. The data represent the mean of triplicate samples, with standard errors shown as vertical bars. There was a significant difference between the dechlorination rates of the two cultures (p < 0.01).
Figure 4. Dechlorination rate (%) in the M-CO and M-CO-B cultures after two weeks of incubation. The bar graphs represent the dechlorination rate calculated based on total organic chloride dechlorinated between Day 0 and Day 14 of incubation as a measure of dechlorination. The data represent the mean of triplicate samples, with standard errors shown as vertical bars. There was a significant difference between the dechlorination rates of the two cultures (p < 0.01).
Ijerph 16 02873 g004
Ijerph 16 02873 g005 550
Figure 5. The effect of H2 on the dechlorination rate (%) after two weeks of incubation, shown in the cultures oxd-H2 and oxd-N2. The bar graphs represent the dechlorination rate calculated based on total organic chloride dechlorinated between Day 0 and Day 14 of incubation as a measure of dechlorination. The data represent the means of triplicate samples, with standard errors shown as vertical bars. There was a significant difference between oxd-H2 and oxd-N2 (p < 0.05).
Figure 5. The effect of H2 on the dechlorination rate (%) after two weeks of incubation, shown in the cultures oxd-H2 and oxd-N2. The bar graphs represent the dechlorination rate calculated based on total organic chloride dechlorinated between Day 0 and Day 14 of incubation as a measure of dechlorination. The data represent the means of triplicate samples, with standard errors shown as vertical bars. There was a significant difference between oxd-H2 and oxd-N2 (p < 0.05).
Ijerph 16 02873 g005
Ijerph 16 02873 g006 550
Figure 6. Microbial composition as identified by 16SrRNA gene sequencing for the M-CO culture. The major population identified for the phyla consisted of 40% Euryarchaeota, 39% Firmicutes, and 16% Proteobacteria. Others include phyla with relative abundance less than 0.5% (namely, spirochaetes, Crenarchaeota, Cyanobacteria, Actinobacteria, OD1, SAR406, and Thermotogae).
Figure 6. Microbial composition as identified by 16SrRNA gene sequencing for the M-CO culture. The major population identified for the phyla consisted of 40% Euryarchaeota, 39% Firmicutes, and 16% Proteobacteria. Others include phyla with relative abundance less than 0.5% (namely, spirochaetes, Crenarchaeota, Cyanobacteria, Actinobacteria, OD1, SAR406, and Thermotogae).
Ijerph 16 02873 g006
Ijerph 16 02873 g007 550
Figure 7. Electron transfer for reductive PCP dechlorination in an autotrophic environment. The figure describes the bioenergetic energy difference associated with autotrophic acetogens and dechlorinators. Here humin in its conductive state acts as the interface for electron transfer from acetate oxidizers (humin reducers) to humin oxidizers as the dechlorinators.
Figure 7. Electron transfer for reductive PCP dechlorination in an autotrophic environment. The figure describes the bioenergetic energy difference associated with autotrophic acetogens and dechlorinators. Here humin in its conductive state acts as the interface for electron transfer from acetate oxidizers (humin reducers) to humin oxidizers as the dechlorinators.
Ijerph 16 02873 g007
Table
Table 1. Experimental setup in this study. HC: homoacetogenic culture; HMBC: humin-dependent PCP-dechlorinating culture; PCP: pentachlorophenol.
Table 1. Experimental setup in this study. HC: homoacetogenic culture; HMBC: humin-dependent PCP-dechlorinating culture; PCP: pentachlorophenol.
Condition NameHumin (1 g)Humin StateMediumHeadspace CompositionComposition of InoculumAdditional Treatment
10% (v/v) HMBC5% (v/v) HC
M-CO+Intactmedium ZH2/CO2++−
CO−−medium ZH2/CO2++−
HC-PCP−−medium ZH2/CO2+−−
Basal+Intactmedium ZH2/CO2−−−
M-CO-B+Intactmedium ZNH2/CO2++−
MCO-Na2S+Intactmedium ZNH2/CO2++1.21 mM Na2S
oxd-H2+Oxidizedmedium ZNH2/CO2++−
oxd-N2+Oxidizedmedium ZNN2/CO2++−
PCP-Sulfate+Intactmedium PCPN2/CO2+−0.5 g/L NA2SO4
PCP-Sal+Intactmedium PCPN2/CO2+−2.25 g/L NaCl
Table
Table 2. Distribution of H2 as milli electron equivalent (meeq) used for electron sinks in acetate production, methane production, sulfate reduction, and PCP dechlorination. *
Table 2. Distribution of H2 as milli electron equivalent (meeq) used for electron sinks in acetate production, methane production, sulfate reduction, and PCP dechlorination. *
Culture NameHydrogen UsedElectron SinkElectron Balance **
Acetate Produced Methane ProducedSulfate ReductionDechlorination
M-CO3.9730.0623.3660.4840.0030.061
M-CO-B3.0820.0672.576-0.0100.429
oxd-H24.9420.4555.096-0.010−0.619
oxd-N2--0.784-0.008−0.776
* The calculation was based on the decrease in headspace H2 as an electron source, and the increase in the product amounts as electron sinks between Day 0 and Day 14. The solubility of the gas was calculated as per the Ostwald dilution law [45]. The calculation of electrons was based on the energetic reactions using hydrogen, as provided in Table S1 [12,25,46,47,48]. ** Positive values suggest the unknown sink, and negative values an unknown electron donor other than H2.

Share and Cite

MDPI and ACS Style

Laskar, M.; Awata, T.; Kasai, T.; Katayama, A. Anaerobic Dechlorination by a Humin-Dependent Pentachlorophenol-Dechlorinating Consortium under Autotrophic Conditions Induced by Homoacetogenesis. Int. J. Environ. Res. Public Health 2019, 16, 2873. https://doi.org/10.3390/ijerph16162873

AMA Style

Laskar M, Awata T, Kasai T, Katayama A. Anaerobic Dechlorination by a Humin-Dependent Pentachlorophenol-Dechlorinating Consortium under Autotrophic Conditions Induced by Homoacetogenesis. International Journal of Environmental Research and Public Health. 2019; 16(16):2873. https://doi.org/10.3390/ijerph16162873

Chicago/Turabian Style

Laskar, Mahasweta, Takanori Awata, Takuya Kasai, and Arata Katayama. 2019. "Anaerobic Dechlorination by a Humin-Dependent Pentachlorophenol-Dechlorinating Consortium under Autotrophic Conditions Induced by Homoacetogenesis" International Journal of Environmental Research and Public Health 16, no. 16: 2873. https://doi.org/10.3390/ijerph16162873

Note that from the first issue of 2016, this journal uses article numbers instead of page numbers. See further details here.

Article Metrics

Back to TopTop