Skip to main content

Aerobic and anaerobic reduction of birnessite by a novel Dietzia strain



Mn oxides occur in a wide variety of geological settings and exert considerable influences on the components and chemical behaviors of sediments and soils. Microbial reduction of Mn oxides is an important process found in many different environments including marine and freshwater sediments, lakes, anoxic basins, as well as oxic-anoxic transition zone of ocean. Although the pathway of Mn anaerobic reduction by two model bacteria, Geobacter and Shewanella, has been intensively studied, Mn bio-reduction is still the least well-explored process in nature. Particularly, reduction of Mn oxides by other bacteria and in the presence of O2 has been fewly reported in recent publishes.


A series of experiments were conducted to understand the capability of Dietzia DQ12-45-1b in bioreduction of birnessite. In anaerobic systems, Mn reduction rate reached as high as 93% within 4 weeks when inoculated with 1.0 × 1010 cells/mL Dietzia DQ12-45-1b strains. Addition of AQDS enhanced Mn reduction rate from 53 to 91%. The anaerobic reduction of Mn was not coupled by any increase in bacterial protein concentration, and the reduction rate in the stable stage of day 2–14 was found to be in good proportion to the protein concentration. The anaerobic reduction of birnessite released Mn(II) either into the medium or adsorbed on the mineral or bacteria surface and resulted in the dissolution of birnessite as indicated by XRD, SEM and XANES. Under aerobic condition, the reduction rate was only 37% with a cell concentration of 1.0 × 1010 cells/mL, much lower than that in parallel anaerobic treatment. Bacterial growth under aerobic condition was indicated by time-course increase of protein and pH. In contrast to anaerobic experiments, addition of AQDS decreased Mn reduction rate from 25 to 6%. The reduced Mn(II) combined with carbon dioxide produced by acetate metabolism, as well as an alkaline pH environment given by cell growth, finally resulted in the formation of Mn(II)-bearing carbonate (kutnohorite), which was verified by XRD and XANES results. The system with the highest cell concentration of 1.0 × 1010 cells/mL gave rise to the most amount of kutnohorite, while concentration of Mn(II) produced with cell concentration of 6.2 × 108 cells/mL was too low to thermodynamically favor the formation of kutnohorite but result in the formation of aragonite instead.


Dietzia DQ12-45-1b was able to anaerobically and aerobically reduce birnessite. The rate and extent of Mn(IV) reduction depend on cell concentration, addition of AQDS or not, and presence of O2 or not. Meanwhile, Mn(IV) bioreduction extent and suspension conditions determined the insoluble mineral products.


Manganese is the 10th most abundant element in the Earth’s crust and second only to iron as the transition metal with alternating redox states [1, 2]. More than 30 kinds of Mn oxide/hydroxide minerals ubiquitously distribute in natural environment [2], which are highly chemically active, and have been recognized as being important in controlling the availability and distribution of many trace metals [26]. Mn cycling depends on various environmental conditions, such as pH, Eh and temperature etc., which lead to complicated behaviors of Mn such as dissolution, precipitation and phase transformation [2, 711]. Microbially influenced transformations of Mn which have been previously reported to take place in soils, sediments, mine tailings, and marine environments, also play an important role in driving geochemical cyclings of Mn [712].

The formation of many naturally occurring Mn oxides is found to be associated with microbial Mn(II) oxidation processes [3, 4, 1315]. Meanwhile, microorganisms were also found to participate in Mn(IV) oxides reduction processes, either by using Mn(IV) as a sole electron acceptor or excreting organics to reduce Mn(IV) as a detoxification mechanism [1618]. Geobacter sp. and Shewanella sp. are two representative species of dissimilatory metal reducing bacteria (DMRB) and have been extensively investigated with respect to their ability to reduce Mn(IV) [10, 16, 1922]. Reduction of Mn(IV) oxides by other DMRB have been seldom reported in recent publishes.

Recent researches carried out the dissimilatory Mn(IV) reduction under anoxic conditions. In the absence of oxygen, some manganese-reducing organisms may use manganese oxides as electron acceptors [16, 17]. While some laboratory studies observed that the presence of oxygen did not inhibit microbial manganese reduction due to the existence of a manganese-reductase system whose activity was inducible by Mn(II) and unaffected by O2 [23, 24]. Although Mn(IV) reduction has been more commonly observed in anaerobic conditions, it may also occur in the presence of oxygen.

Factually, biotic manganese reduction is complicated in natural environments and is found to be influenced by various factors. Besides the types of microbial species and O2 level, electron shuttles, such as humic acid and quinone-containing compounds, also have great influences on microbial Mn(IV) reduction rates [18, 25, 26]. Lovley [25] proved that addition of humic substances or anthraquinone-2,6-disulfonate (AQDS) greatly stimulated the reduction activity of Geobacter metallireducens. Ruebush [26] testified that enzymatic reduction of Mn oxides by membrane fractions from Shewanella oneidensis MR-1 was accelerated with addition of AQDS.

In this study, a fermentative facultative anaerobe, Dietzia strain DQ12-45-1b, which was isolated from a microaerobic condition, was investigated for reduction of a most common Mn(IV) oxide, birnessite. Given previously reported observations, microbial Mn(IV) reduction by DQ12-45-1b were further studied by examining possible constrains of cell densities, O2 and electron shuttles (AQDS) on Mn(IV) reduction rates as well as the resulting Mn-bearing mineral products.


Birnessite preparation

Birnessite was synthesized using the method described by McKenzie [27]. A 30 mL concentrated HCl (AR) was added dropwisely with stirring to a boiling solution containing 0.2 mol KMnO4 (AR) dissolved in 350–400 mL of water. After all 30 mL HCl added into the KMnO4 solution, the reaction was continued under another 30 min boiling. The precipitate was filtered and washed 15 times with deionized water [18 MΩ conductivity (Reference, Merck Milipore, Germany)] to remove K+ and Cl possibly adsorbed on the mineral surface. The resulting precipitate was dried in air at 45°C over night and then stored for further test and experiment.


Dietzia strain DQ12-45-1b was isolated from oil production water in a deep subterranean oil-reservoir of an oilfield in China [28]. This strain was gram-positive, facultatively anaerobic, non-motile with no flagellum and had the ability to degradation of petroleum hydrocarbons [28]. Batch growth experimental data showed DQ12-45-1b was able to grow on any single substrate of succinate, acetate and glucose, while formate, lactate and citrate could not serve as the sole carbon and energy source for bacterial growth. Therefore, we chose a simple organic of acetate as the electron donor in this study.

The strain was prepared for bioreduction experiments after aerobic enrichment cultivation in Luria–Bertani medium (LB medium, 10 g/L of peptone, 5 g/L of yeast extract and 10 g/L of NaCl) under ambient condition. In bioreduction experiments, strain DQ12-45-1b was cultured anaerobically or aerobically in a medium [29] consisting of (per liter): 6.56 g sodium acetate, 1.19 g (NH4)2SO4, 0.1 g MgSO4, 0.043 g CaCl2, 0.0012 g FeSO4, and 20 mM HEPES buffer at 35°C.

Bioreduction experiments

Birnessite (final concentration = 0.3 mg/mL) was suspended with the culture medium in serum bottles sealed with blue butyl rubber stoppers (for anaerobic) and in flasks (for aerobic) with total volume of 80 mL. In anaerobic experiments, the medium used for anaerobic cultures was made anoxic in serum bottles with O2-free N2/CO2 gasmix (80:20) and sterilized by autoclaving. Dietzia DQ12-45-1b cell was enriched from LB medium by centrifugation at 4,024g, and then washed with sterilized culture medium. This procedure was repeated for three times to remove LB medium, and then the cell pellet was suspended with sterilized culture medium and injected into serum bottles with a fixed concentration. In selected experiments, 0.1 mM anthraquinone-2,6-disulfonate (AQDS) was supplied as an electron shuttle. AQDS solution and HEPES buffer were sterilized by filtration with 0.22 μm Millipore filter and injected into the medium with syringes. The control group was identical to the experimental bottles except that cells were replaced with an equal amount of the culture medium (sterile control) or inactivated cells (killed control). All treatments were performed in duplicates. All vials were incubated in a constant temperature shaking table at 35°C. Samplings were conducted in certain time interval in glove box (855AC, Plas-Labs, USA). 3 mL of suspensions was taken out for pH, Mn2+ concentration and protein concentration tests to evaluate microbial reduction and the changes of biomass. In aerobic experiments, all processes were identical to those in anaerobic experiments except that oxygen removal was not conducted and the sampling processes were conducted in super clean bench.

Analytical methods

Mn2+ concentration (C l ) was measured by ICP-OES (Spectroblue, Spectro, Germany) after removing solids by centrifugation of 1 mL cell-mineral suspension. Protein concentrations were measured by Bradford method [30]. 1 mL sample was centrifuged at 9,391g and the supernatant was discarded. 0.2 M NaOH was fully mixed with cell pellet, and the mixture was boiled for 12 min to breakdown the cells and release proteins. The alkali treated sample was then centrifuged and the protein fraction in the supernatant was quantified with the Bradford assay using the standard curve established by bovine serum albumin (BSA) as a standard [30].

Mn average oxidation state (AOS) of the suspensions was calculated after measuring the total Mn content, Mn2+ content in the medium and Mn(III)/Mn(IV) content, respectively. First, total Mn content (C total ) was measured by dissolving 0.5 mL suspension using 2 mL 0.25 M hydroxylamine hydrochloride, then diluted to 10 mL with 2% HNO3, and then the Mn concentration was determined by ICP-OES. Aqueous Mn2+ content (C l ) in the solution was also determined by ICP-OES. The amount of Mn(IV) in the suspension was measured by reaction with the reductive dye, Leucober-belin blue I (LBB) using the standard curve established by KMnO4 as a standard [31]. Oxidized LBB is blue and the color intensity is a function of the amount of Mn(III)/Mn(IV) being reduced to Mn(II). The color intensity was measured for optical density at 620 nm using the spectrophotometer. Amount of electron transfer between Mn(III)/Mn(IV) and Mn(II) was noted as Ne. A concentration of 10 μM KMnO4 equaled 50 μM electron transfer. According to the amount of total Mn, Mn2+ and transfer electrons, the Mn AOS was calculated as following equations:

$$ {\text{AOS}}_{{({\text{Total Mn}})}} = { 2} + {\text{N}}_{e} /{\text{C}}_{total} $$
$$ {\text{AOS}}_{{({\text{insoluble Mn}})}} = { 2} + {\text{N}}_{e} /\left( {{\text{C}}_{total} - {\text{ C}}_{l} } \right) $$

where AOS(Total Mn) means AOS of total Mn in the suspensions and AOS(insoluble Mn) means AOS of insoluble Mn including Mn in minerals and adsorbed on bacteria or minerals.

It is supposed that all Mn(III)/Mn(IV) were reduced to Mn(II). And birnessite reduction rate was calculated as following:

$$ {\text{Reduction extent }} = \left( {{\text{AOS}}_{\text{({{Total Mn}})}t} - 2} \right)/ \, \left( {{\text{AOS}}_{{\left( {\text{Total Mn}} \right){\it 0}}} - 2} \right) \times 100\% $$

where AOS(Total Mn)0 means AOS of total Mn at the original time and AOS(Total Mn)t means AOS of total Mn after reaction. AOS(Total Mn)0 was measured as 3.92.

Mineral characterization

Mineralogical changes after bioreduction were determined by powder X-ray diffraction (XRD). XRD patterns were recorded using X`pert powder diffractometer (PANalytical B.V., the Netherlands) with CuKα radiation (λ = 0.15406 nm). The instrument was operated at a tube voltage of 40 kV and a tube current of 40 mA. Intensities were measured at 2θ = 5°–70° with 0.02° two-theta steps and a count time of 0.3 s per step.

The mineral micro-morphologies were further characterized by scanning electron microscopy (SEM). Suspensions (1 mL) were washed by deionized water to remove medium on the mineral surface. The samples were dispersed on polished silicon wafer and then mounted on an aluminum SEM stub via conductive tapes and coated with gold using a Denton Desk II Gold Sputter Coater for SEM observations. The samples were observed under a FEI Quanta 200F SEM with an X-ray energy dispersive spectroscopy (SEM/EDS). The SEM was operated at an accelerating voltage of 10 or 15 kV.

The X-ray absorption near-edge data (XANES) at the Mn K-edge of the original and bioreduced samples were recorded at room temperature in transmission mode using ion chambers at beam line BL14W1 of the Shanghai Synchrotron Radiation Facility (SSRF), China. The station was operated with a Si (111) double crystal monochromator with a resolution of 1.3 × 10−4 eV. Mn K-edge XANES data were collected over the energy range 6,339–6,839 eV in transmission mode. Each powder sample was sandwiched between two pieces of KAPTON tape located on the beam path. During the measurement, the synchrotron was operated at energy of 3.5 GeV and a maximum current of 250 mA. The photon energy was calibrated with the first inflection point of Mn K-edge in Mn metal foil. Data reduction of experimental XANES spectra was carried out using the software ATHANE 1.2.11. Pre-edge background subtraction and XANES normalization were carried out by fitting a linear polynomial to the pre-edge region and a quadratic polynomial to the postedge region of the absorption spectrum.

Results and discussion

Anaerobic reduction of birnessite by DQ12-45-1b

The results of birnessite reduction by DQ12-45-1b were shown in Fig. 1 and summarized in Table 1. As observed in Fig. 1a, significant amounts of Mn2+ were produced in bacterial treatments, which was considerably higher than the concentrations of Mn2+ in sterile control and killed control. In the initial 14 days, the amounts of Mn2+ increased with time and 6, 21 and 42% of Mn(IV) was reduced with the initial cell concentration of 6.2 × 108, 2.5 × 109 and 1.0 × 1010 cells/mL, respectively. By contrast, the chemical reduction extent of Mn(IV) by acetate was below 5%.

Fig. 1

Aqueous Mn2+ concentrations (a) and protein concentrations (solid symbol)/pH values (hollow symbol) (b) during anaerobic birnessite reduction with different initial cell concentrations.

Table 1 Anaerobic reduction of birnessite under different cell concentrations

Since changes in Mn reduction rate could be roughly estimated from Mn2+ release rate, three stages of Mn reduction process could be approximately obtained from Fig. 1a. The first stage is the initial 2 days, when Mn2+ concentration increased but with a relatively lower rate than the following several days. Mn2+ release rates with initial cell concentrations of 6.2 × 108 and 2.5 × 109 during 2–14 days and that with 1.0 × 1010 cells/mL during 2–10 days was calculated to be 12.2, 48.0 and 114.9 μM/day, respectively, showing a positive correlation with the inoculated cell density. However, Mn2+ release rates after 14 days decreased to 9.1 and 26.5 μM/day in the treatments with two lower cell concentrations, indicating the bacterial activity associated with Mn bioreduction went down. Even a slight decrease in Mn2+ concentration after 14 days was observed with the highest inoculation concentration of 1.0 × 1010 cells/mL, suggesting the bioreduction possibly stopped. Besides, tiny amounts of particles were observed in the medium after 14 days. All these evidences indicated the bioreduction of Mn with the highest cell concentration of 1.0 × 1010 cells/mL was close to completion at the 14th day. Consistently, the AOS of the residuals were measured to be 2.22 (Table 1) and found to be approaching 2. The slight decrease of Mn2+ concentration after 14 days would be explained by adsorption of Mn(II) onto the cell or residual mineral surface, or else by forming Mn(II)/Mn(III) minerals [3234]. So, in bacterial treatment with cell concentration of 1.0 × 1010 cells/mL, almost all Mn(IV) in birnessite was reduced to Mn(II) after 14 days and part of produced Mn(II) was present as insoluble state. There was a positive relationship between the Mn reduction rate and the cell concentration, that the final reduction extent of birnessite was 33, 53 and 93% (Fig. 1; Table 1), corresponding to the cell concentration of 6.2 × 108, 2.5 × 109 and 1.0 × 1010 cells/mL, respectively.

Previous studies showed Shewanella oneidensis MR-1 could couple its anaerobic growth to Mn(IV) reduction and gain energy from the redox reaction including organics oxidation and metal reduction [16]. Here, acetate served as the electron donor, and birnessite served as the electron acceptor. So, the total reaction could be given as:

$$ 3 {\text{MnO}}_{ 2} + {\text{ CH}}_{ 3} {\text{COO}}^{ - } + {\text{ H}}_{ 2} {\text{O}} \mathop{\longrightarrow}\limits 3 {\text{Mn}}^{ 2+ } + {\text{ 2HCO}}_{ 3}^{ - } + {\text{ 3OH}}^{ - } $$

However, the anaerobic reduction of birnessite by DQ12-45-1b were found to be unaccompanied by bacterial growth. In the presence of birnessite as the sole electron acceptor, the concentrations of Mn2+ continuously increased in all three bacterial treatments during the stable bioreduction stage (day 2–14), while the bacterial protein concentration kept stable (Fig. 1b). Particularly, the Mn2+ release rates were found to be in good proportion to the protein concentrations (Fig. 2). Therefore, we can confirm the anaerobic reduction of birnessite by DQ12-45-1b was not a direct biological process linking Mn reduction with bacterial growth. Considering the results of killed control and the positive correlation between the Mn2+ release rates and protein concentrations, we speculate the bioreduction process may be an enzymatic reaction, which needs further demonstration.

Fig. 2

A positive relationship between protein and Mn2+ release rate (abscissa values were the mean values of proteins in 2–14 days).

Aerobic reduction of birnessite by DQ12-45-1b

Under aerobic conditions, Mn2+ concentration of sterile treatment gradually increased over the experiment (Fig. 3a) due to acetate reduction. In treatments with the initial inoculation cell concentration of 6.2 × 108, 2.5 × 109 and 1.0 × 1010 cells/mL, Mn2+ concentration in the initial 2 days sharply increased to 33.0, 98.7 and 180.0 μM, respectively. The initial Mn2+ release rates also showed a positive correlation with the inoculated cell density. Meanwhile, the pH drastically went up from 6.9 to 8.3 for the two higher cell concentrations even in the presence of HEPES buffer, which lead to the quick precipitation, re-adsorption of Mn(II) on the mineral surface or re-oxidation of Mn(II) as reflected by the abrupt drop of Mn2+ concentration to zero in the following days. As expected, some white precipitations were observed in the suspensions with two higher cell concentrations of 2.5 × 109 and 1.0 × 1010 cells/mL, indicating the formation of new minerals related to Mn reduction. In the medium with the lowest cell concentration of 6.2 × 108 cells/mL, both the maximum Mn2+ generation and the most drastic change in pH were recorded later than in the equivalent treatments with higher cell concentration (approximately at the 6th day). And after the 6th day, the Mn2+ concentration did not undergo a sudden change to zero but gradually decreased. No visible precipitates were observed in this treatment.

Fig. 3

Aqueous Mn2+ concentration (a) and protein concentration (solid symbol)/pH value (hollow symbols) (b) during aerobic birnessite reduction with different initial cell concentration.

Bacterial growth under aerobic condition was indicated by time-course increase of protein and pH (Fig. 3b). When grown in pure culture with O2 as the terminal electron acceptor, the DQ12-45-1b strains were found to be able to increase the pH value from neutral to alkaline scales (data not shown). Therefore, the rapider increase in both soluble Mn2+ and pH values in bacterial treatments than those in sterile control, as well as the obvious positive correlation between the inoculated cell concentration and Mn reduction extent indicated the aerobic Mn reduction was correlated with the bacterial growth. In a separate experimental batch, which was to examine the relationship between the acetate consumption and cell concentration, we observed the depletion of acetate at around the 6th day (Additional file 1: Figure S1). So, along with the depletion of carbon source, the bacterial growth stagnated, and the protein concentration did not increase any more (Fig. 3b). The pH went stable and finally maintained at 9.6–9.7 (Fig. 3b).

After 24 days, the AOS of insoluble Mn in the system with initial cell concentrations of 2.5 × 109 and 1.0 × 1010 cells/mL were 3.44 and 3.21, corresponding to 25 and 37% of Mn reduction, respectively (Table 2). The actual Mn reduction extent should be higher than the experimental values, because under alkaline condition, re-oxidation of Mn(II) by O2 is feasible [35, 36]. In comparison, the AOS of insolubles with initial cell concentration of 6.2 × 108 cells/mL was 3.92 (Table 2), the same as the original birnessite. Although there were some Mn2+ continuously released in the initial 6 days of 6.2 × 108 cells/mL treatment, the Mn2+ concentration gradually decreased in the following days (Fig. 3a).

Table 2 Aerobic reduction of birnessite under different cell concentrations

Comparing Mn bioreduction in the presence and absence of O2, it could be found that Mn reduction extents under aerobic condition were much lower than those under anaerobic conditions, although stain DQ12-45-1b grew more vigorous under aerobic conditions. These findings suggested O2 interfered with birnessite reduction, not only as an alternative electron acceptor to compete with Mn(IV) reduction, but also as an oxidizer leading to re-oxidation of Mn(II) in alkaline pH.

Effect of AQDS on reduction of birnessite

Addition of the humic acid analog AQDS generally enhanced Mn2+ release rates under anaerobic condition (Fig. 4a). The Mn2+ release rate with AQDS was observed to be approximately one time higher than that without AQDS in the initial 2–14 days and more than 60% higher in 14–28 days (Table 3). Consistently, the AOS of the insolubles decreased from the initial 3.92 to 2.57 with AQDS and to 3.35 without AQDS.

Fig. 4

Aqueous Mn2+ concentration during birnessite reduction with/without AQDS under anaerobic condition (a) and aerobic condition (b).

Table 3 Microbial Mn reduction with or without AQDS

Under aerobic condition, a slight enhancement of Mn2+ release rates was observed in the presence of AQDS in the first 2 days (Fig. 4b). However, unlike in anaerobic experiments, the addition of AQDS did not enhance the Mn reduction extent, and the AOS of the insolubles was 3.80 with AQDS and 3.44 without AQDS (Table 3).

It is believed that AQDS could enhance the rate and extent of microbial metal reduction by shuttling electrons from bacteria to mineral surfaces and thus eliminating the requirement for direct contact of bacteria with electron acceptors [18, 3740]. The possible reduction of AQDS by cells gave rise to biogenic AH2DS (reduced state of AQDS), which then undertook chemical reduction of Mn(IV) [38, 40]. This mechanism could explain the observed increase in both the rate and extent of Mn reduction under anaerobic condition. Under aerobic condition, electrons were transferred to AQDS prior to birnessite and O2 [41]. Birnessite and O2 competed to accept electrons from biogenic AH2DS. At neutral to alkaline environment, the redox potential of O2 was higher than that of birnessite, especially at alkaline pH (Fig. 5). So the biogenic AH2DS may be preferentially to be oxidized by O2. In aerobic bio-treatment, AQDS as an electron shuttle essentially accelerated electron transfer between bacteria and O2, which finally lead to the inhibition of Mn(IV) reduction.

Fig. 5

Reduction potential of O2, birnessite (at 2 × 10−5 and 2 × 10−6 M Mn2+ activity) [42] and AQDS (at 5 × 10−5 M AQDS plus 5 × 10−5 M AH2DS and 10−4 AQDS M plus 10−7 M AH2DS activity) [43] as a function of pH.

Mineral characterization of bioreduced samples

Under anaerobic condition, no visible color change in the residual insolubles was observed and the quantity of insoluble in bio-treatments obviously decreased after the experiments. The XRD patterns of residuals in all anaerobic bio-treatments showed the characteristic peaks of birnessite (JCPDS: 23-1239) (Fig. 6a), but with significant loss in peak strength as compared to sterile controls, which was in agreement with the visual observations of bio-induced dissolution of birnessite. No other secondary minerals were detected by XRD.

Fig. 6

XRD patterns of bioreduced samples under anaerobic (a) and aerobic condition (b).

It was also found that the peak strength decreased as the cell concentration increased, which was attributed to the improved reduction extent of birnessite by higher cell concentration (Fig. 1; Table 1). Besides, the addition of AQDS also significantly accelerated the microbial Mn reduction (Fig. 4a), thereby resulted in more complete dissolution of birnessite and poorer quality XRD patterns of residuals (Fig. 6a).

Further, by comparing the XANES spectra of the residuals in anaerobic bio-treatment to the original birnessite (Fig. 7), we can find a similar peak assigned to Mn(IV) at 6,562 eV and a weak shoulder assigned to Mn(II) at 6,552 eV [44, 45], the latter of which was probably ascribed to adsorbed Mn(II) from birnessite reduction. Taken together, all these data demonstrated the anaerobic reduction of birnessite by DQ12-45-1b released Mn(II) and caused the dissolution of birnessite.

Fig. 7

XANES spectra of original birnessite and bioreduced samples in the system with an initial cell concentration of 2.5 × 109 cells/mL.

In aerobic bio-treatments, white suspensions in strong color contrast to black birnessite were observed, indicating the possible precipitation of new mineral phases. Under SEM, some spindle-like aggregations were found and their surface appeared with many holes whose size and shape were very similar to a single cell (Fig. 8b). The EDS results (Fig. 8c) indicated the aggregations mainly consisted of Mg, Ca, Mn, C and O, which was very different from the composition of birnessite. Consistently, XRD patterns of aerobic bioreduced samples showed several new peaks at 2θ = 2.39°, 30.8° and 50.7°, which were assigned to (012), (104) and (\(1{\bar{1}}6\)) reflections of kutnohorite [Ca(Mn,Mg)(CO3)2; JCPDS: 084-1290], respectively (Fig. 6b). Thereafter, an obvious shoulder feature at approximately 6,552 eV in the XANES spectra of the residuals in aerobic bio-treatment verified the formation of Mn(II)-bearing minerals.

Fig. 8

SEM of original and bioreduced samples. a SEM of original globular-flower-like birnessite; b SEM of spindle-shape mineral after microbial reduction under aerobic condition; c EDS of spindle-shape mineral after microbial reduction under aerobic condition.

With the growth of stain DQ12-45-1b, carbon dioxide accumulation from the oxidation of acetate and the increased pH value caused high CO3 2− activity, therefore leading to the precipitation of carbonate minerals. Accordingly, the quantity of produced carbonates was positively associated with the inoculated cell concentration (Fig. 6b). Surprisingly, only the sample with the lowest cell concentration of 6.2 × 108 cells/mL did not show any peaks of kutnohorite, but showed the existence of aragonite (CaCO3; JCPDS: 05-0453) (Fig. 6b). This phenomenon was in agreement with the considerably low concentration of Mn2+ (Fig. 3a) and high value of AOS (Table 2) as measured before. Mn(II) produced by bioreduction combined with carbon dioxide produced by acetate metabolism, as well as an alkaline pH environment given by cell growth, finally resulted in the formation of Mn(II)-bearing carbonate (kutnohorite). The concentration of Mn(II) produced in bio-treatment with cell concentration of 6.2 × 108 cells/mL was too low to thermodynamically favor the formation of kutnohorite. And the insufficient supply of Mn(II) resulted in the formation of aragonite instead. Although Mn(II) re-oxidation by O2 competed with Mn reduction in aerobic treatments, once the net content of produced Mn(II) reached a proper level, Mn(II) would quickly precipitate and not allow for further oxidation by O2. This point could be drawn from the two bio-systems with higher cell concentration. Accordingly, the system with the highest cell concentration of 1.0 × 1010 cells/mL gave rise to the most amount of kutnohorite as indicated by XRD results (Fig. 6b). Since DQ12-45-1b preferentially transferred electrons to AQDS and the presence of AQDS facilitated O2 reduction but interfered Mn reduction, a relatively smaller proportion of kutnohorite was obtained in the presence of AQDS as compared to that without addition of AQDS (Fig. 6b).


Birnessite reduction in presence of DQ12-45-1b was observed in both anaerobic and aerobic conditions, and the Mn(IV) reduction proceeded at a more rapid rate when inoculated with higher cell concentration. The extent of Mn(IV) reduction in aerobic conditions was lower than that in anaerobic conditions due to the re-oxidation by oxygen or competition with oxygen respiration. In anaerobic conditions, addition of AQDS improved Mn(IV) reduction extent and accelerated Mn(II) production rate, which ultimately promoted birnessite dissolution. In aerobic treatments, indirect effects ascribed from bacterial metabolism, such as changes of pH, consumption of oxygen and release of metabolites etc., gave a profound influence on the balance between Mn(IV) reduction and Mn(II) re-oxidation, which ultimately lead to the final AOS of Mn oxides, and decided the insoluble products. The presence of AQDS and O2 was demonstrated to interfere Mn(IV) reduction and result in low reduction extent of birnessite. The formation of Mn(II)-bearing carbonate (kutnohorite) in aerobic conditions depended on how fast and how far birnessite was reduced to give rise to Mn(II) available for precipitation.


  1. 1.

    Turekian KK, Wedepohl KH (1961) Distribution of the elements in some major units of the Earth’s crust. Geol Soc Am Bull 72:175–192

    Article  Google Scholar 

  2. 2.

    Post JE (1999) Manganese oxide minerals: crystal structures and economic and environmental significance. Proc Natl Acad Sci USA 96:3447–3454

    Article  Google Scholar 

  3. 3.

    Nelson YM, Lion LW (2003) Formation of biogenic manganese oxides and their influence on the scavenging of toxic trace metals. In: Selim HM, Kingerly WL (eds) Geochemical and hydrological reactivity of heavy metals in soils. CRC Press, Boca Raton, pp 169–186

    Google Scholar 

  4. 4.

    Tebo BM, Bargar JR, Clement BG, Dick GJ, Murray KJ, Parker D et al (2004) Biogenic manganese oxides: properties and mechanisms of formation. Annu Rev Earth Pl Sc 32:287–328

    Article  Google Scholar 

  5. 5.

    O’Reilly SE, Hochella MF (2003) Lead sorption efficiencies of natural and synthetic Mn and Fe-oxides. Geochim Cosmochim Acta 67:4471–4487

    Article  Google Scholar 

  6. 6.

    Sherman DM, Peacock CL (2010) Surface complexation of Cu on birnessite (d-MnO2): controls on Cu in the deep ocean. Geochim Cosmochim Acta 74:6721–6730

    Article  Google Scholar 

  7. 7.

    White JR, Driscoll CT (1987) Manganese cycling in an acidic Adirondack lake. Biogeochemistry 3:87–103

    Article  Google Scholar 

  8. 8.

    Slomp CP, Malschaert JFP, Lohse L, Van Raaphorst W (1997) Iron and manganese cycling in different sedimentary environments on the North Sea continental margin. Cont Shelf Res 17:1083–1117

    Article  Google Scholar 

  9. 9.

    Ukrainczyk L, McBride MB (1992) Oxidation of phenol in acidic aqueous suspensions of manganese oxide. Clay Clay Miner 40:157–166

    Article  Google Scholar 

  10. 10.

    Lovley DR (1993) Dissimilatory metal reduction. Annu Rev Microbiol 7:263–290

    Article  Google Scholar 

  11. 11.

    Lovley DR, Holmes DE, Nevin KP (2006) Dissimilatory Fe (lII) and Mn (lV) reduction. Adv Microb Physiol 49:219–286

    Article  Google Scholar 

  12. 12.

    Jones C, Crowe SA, Sturm A, Leslie KL, Maclean LCW, Katsev S et al (2011) Biogeochemistry of manganese in ferruginous lake matano, indonesia. Biogeosciences 8:2977–2991

    Article  Google Scholar 

  13. 13.

    Bargar JR, Tebo BM, Bergmann U, Webb SM, Glaetzel P, Chiu VQ et al (2005) Biotic and abiotic products of Mn(II) oxidation by spores of the marine Bacillus sp. strain SG-1. Am Mineral 90:143–154

    Article  Google Scholar 

  14. 14.

    Jürgensen A, Widmeyer JR, Gordon RA, Bendell-Young LI, Moore MM, Crozier ED (2004) The structure of the manganese oxide on the sheath of the bacterium Leptothrix discophora: an XAFS study. Am Mineral 89:1110–1118

    Google Scholar 

  15. 15.

    Villalobos M, Bargar JR, Sposito G (2005) Trace metal retention on biogenic manganese oxide nanoparticles. Elements 1:223–226

    Article  Google Scholar 

  16. 16.

    Myers CR, Nealson KH (1988) Bacterial manganese reduction and growth with manganese oxide as the sole electron acceptor. Science 240:1319–1321

    Article  Google Scholar 

  17. 17.

    Lovley DR, Phillips EJP (1988) Novel mode of microbial energy metabolism: organic carbon oxidation coupled to dissimilatory reduction of iron or manganese. Appl Environ Microbiol 54:1472–1480

    Google Scholar 

  18. 18.

    Lovely D (2013) Dissimilatory Fe(III)-and Mn(IV)-reducing prokaryotes. In: Rosenberg E, DeLong EF, Lory S, Stackebrandt E, Thompson F (eds) The prokaryotes. CBS Publishers, New Delhi, pp 287–308

    Google Scholar 

  19. 19.

    Mehta T, Coppi MV, Childers SE, Lovley DR (2005) Outer membrane c-type cytochromes required for Fe(III) and Mn(IV) oxide reduction in Geobacter sulfurreducens. Appl Environ Microbiol 71:8634–8641

    Article  Google Scholar 

  20. 20.

    Aklujkar M, Coppi MV, Leang C, Kim BC, Chavan MA, Perpetua LA et al (2013) Proteins involved in electron transfer to Fe(III) and Mn(IV) oxides by Geobacter sulfurreducens and Geobacter uraniireducens. Microbiology 159:515–530

    Article  Google Scholar 

  21. 21.

    Kouzuma A, Hashimoto K, Watanabe K (2012) Roles of siderophore in manganese-oxide reduction by Shewanella oneidensis MR-1. FEMS Microbiol Lett 326:91–98

    Article  Google Scholar 

  22. 22.

    Shi L, Squier TC, Zachara JM, Fredrickson JK (2007) Respiration of metal (hydr)oxides by Shewanella and Geobacter: a key role for multihaem c-type cytochromes. Mol Microbiol 65:12–20

    Article  Google Scholar 

  23. 23.

    Ghiorse WC (1984) Biology of iron and manganese depositing bacteria. Annu Rev Microbiol 38:515–550

    Article  Google Scholar 

  24. 24.

    Trimble RB, Ehrlich HL (1970) Bacteriology of manganese nodules. IV. Induction of a MnO2-reductase system in a marine bacillus. Appl Microbiol 19:966–972

    Google Scholar 

  25. 25.

    Lovley DR, Coates JD, Blunt-Harris EL, Phillips EJP, Woodward JC (1996) Humic substances as electron acceptors for microbial respiration. Nature 382:445–448

    Article  Google Scholar 

  26. 26.

    Ruebush SS, Icopini GA, Brantley SL, Tien M (2006) In vitro enzymatic reduction kinetics of mineral oxides by membrane fractions from Shewanella oneidensis MR-1. Geochim Cosmochim Acta 70:56–70

    Article  Google Scholar 

  27. 27.

    McKenzie RM (1971) The synthesis of birnessite, cryptomelane, and some other oxides and hydroxides of manganese. Mineral Mag 38:493–502

    Article  Google Scholar 

  28. 28.

    Wang XB, Chi CQ, Nie Y, Tang YQ, Tan Y, Wu G et al (2011) Degradation of petroleum hydrocarbons (C6–C40) and crude oil by a novel Dietzia strain. Bioresour Technol 102:7755–7761

    Article  Google Scholar 

  29. 29.

    Kostka JE, Luther GW, Nealson KH (1995) Chemical and biological reduction of Mn(III)-pyrophosphate complexes epotential importance of dissolved Mn(III) as an environmental oxidant. Geochim Cosmochim Acta 59:885–894

    Google Scholar 

  30. 30.

    Zor T, Selinger Z (1996) Linearization of the Bradford protein assay increases its sensitivity: theoretical and experimental studies. Anal Biochem 236:302–308

    Article  Google Scholar 

  31. 31.

    Krumbein WE, Altmann HJ (1973) A new method for the detection and enumeration of manganese oxidizing and reducing microorganisms. Helgolinder wiss Meeresunters 25:347–356

    Article  Google Scholar 

  32. 32.

    Fischer TB, Heaney PJ, Jang JH, Ross DE, Brantley SL, Post JE et al (2008) Continuous time-resolved X-ray diffraction of the biocatalyzed reduction of Mn oxide. Am Mineral 93:1929–1932

    Article  Google Scholar 

  33. 33.

    Bratina BJ, Stevenson BS, Green WJ, Thomas MS (1998) Manganese reduction by microbes from oxic regions of the lake Vanda (Antarctica) water column. Appl Environ Microbiol 64:3791–3797

    Google Scholar 

  34. 34.

    Burdige DJ, Nealson KH (1985) Microbial manganese reduction by enrichment cultures from coastal marine sediments. Appl Environ Microbiol 50:491–497

    Google Scholar 

  35. 35.

    Fendorf SE, Sparks DL, Franz JA, Camaioni DM (1993) Electron paramagnetic resonance stopped-flow kinetic study of manganese sorption-desorption on birnessite. Soil Sci Soc Am J 57:57–62

    Article  Google Scholar 

  36. 36.

    Yang DS, Wang MK (2002) Synthesis and characterization of birnessite by oxidizing pyrochroite in alkaline conditions. Clay Clay Miner 50:63–69

    Article  Google Scholar 

  37. 37.

    Fredrickson JK, Zachara JM, Kennedy DW, Dong H, Onstott TC, Hinman NW et al (1998) Biogenic iron mineralization accompanying the dissimilatory reduction of hydrous ferric oxide by a groundwater bacterium. Geochim Cosmochim Acta 62:3239–3257

    Article  Google Scholar 

  38. 38.

    Jaisi DP, Dong H, Liu C (2007) Influence of biogenic Fe(II) on the extent of microbial reduction of Fe(III) in clay minerals nontronite, illite, and chlorite. Geochim Cosmochim Acta 71:1145–1158

    Article  Google Scholar 

  39. 39.

    Liu C, Zachara JM, Foster NS, Strickland J (2007) Kinetics of reductive dissolution of hematite by bioreduced anthraquinone-2,6-disulfonate. Environ Sci Technol 41:7730–7735

    Article  Google Scholar 

  40. 40.

    Burgos WD, Fang Y, Royer RA, Yeh GT, Dempsey BA (2003) Reaction-based modeling of quinone-mediated bacterial iron(III) reduction. Geochim Cosmochim Acta 67:2735–2748

    Article  Google Scholar 

  41. 41.

    Brose DA, James BR (2010) Oxidation-reduction transformations of chromium in aerobic soils and the role of electron-shuttling quinones. Environ Sci Technol 44:9438–9444

    Article  Google Scholar 

  42. 42.

    Briker O (1965) Some stability relations in the system Mn–O2–H2O at 25°C and one atmosphere total pressure. Am Mineral 50:1296–1354

    Google Scholar 

  43. 43.

    Clark WM (1960) Oxidation-reduction potential of organic systems. The Williams and Wilkins Co, Baltimore

    Google Scholar 

  44. 44.

    Villalobos M, Toner B, Bargar J, Sposito G (2003) Characterization of the manganese oxide produced by Pseudomonas putida strain MnB1. Geochim Cosmochim Acta 67:2649–2662

    Article  Google Scholar 

  45. 45.

    Webb SM, Tebo BM, Bargar JR (2005) Structural characterization of biogenic Mn oxides produced in seawater by the marine bacillus sp. strain SG-1. Am Mineral 90:1342–1357

    Article  Google Scholar 

Download references

Authors’ contributions

HZ co-planned experiments, carried out the experiments and drafted the manuscript. YL co-planned experiments, did revision and gave final approval of the version to be published. XW, HD and CZ contributed to the interpretation of the results and helped polish the manuscript. AL participated in the design of the study and funded the study. CW helped design the study. XW helped carry out the analyses of Mn concentration. YN and XW isolated the bacteria. All authors read and approved the final manuscript.


This work was funded by the National Basic Research Program of China (973 Program) (Grant no. 2014CB846001) and the National Natural Science Foundation of China (Grant no. 41230103, 41272003 and 41402032). The authors thank beamline BL14W1 (Shanghai Synchrotron Radiation Facility) for providing the beam time.

Compliance with ethical guidelines

Competing interests The authors declare that they have no competing interests.

Author information



Corresponding author

Correspondence to Anhuai Lu.

Additional information

Huiqin Zhang and Yan Li contributed equally to this work

Additional file

Additional file 1:

Figure S1. Acetate concentrations during aerobic birnessite reduction with different initial cell concentrations.

Rights and permissions

Open Access This article is distributed under the terms of the Creative Commons Attribution 4.0 International License (, which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver ( applies to the data made available in this article, unless otherwise stated.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Zhang, H., Li, Y., Wang, X. et al. Aerobic and anaerobic reduction of birnessite by a novel Dietzia strain. Geochem Trans 16, 11 (2015).

Download citation


  • Shewanella
  • XANES Spectrum
  • Initial Cell Concentration
  • Electron Shuttle
  • High Cell Concentration