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Accepted Manuscript
Title: ISOLATION AND BIOELECTROCHEMICALCHARACTERIZATION OF NOVEL FUNGAL SOURCES
WITH OXIDASIC ACTIVITY APPLIEDIN-SITUFOR THE
CATHODIC OXYGEN REDUCTION IN MICROBIAL
FUEL CELLS
Author: Kyriale Vasconcelos Morant Paulo Henrique da Silva
Galba Maria de Campos-Takaki Camilo Enrique La Rotta
Hernandez
PII: S0141-0229(14)00137-9
DOI: http://dx.doi.org/doi:10.1016/j.enzmictec.2014.07.007Reference: EMT 8665
To appear in: Enzyme and Microbial Technology
Received date: 28-5-2014
Revised date: 14-7-2014
Accepted date: 25-7-2014
Please cite this article as: Morant KV, Silva PH, Campos-Takaki GM, Hernandez CELR,
ISOLATION AND BIOELECTROCHEMICAL CHARACTERIZATION OF NOVEL
FUNGAL SOURCES WITH OXIDASIC ACTIVITY APPLIED IN-SITUFOR THECATHODIC OXYGEN REDUCTION IN MICROBIAL FUEL CELLS., Enzyme and
Microbial Technology(2014),http://dx.doi.org/10.1016/j.enzmictec.2014.07.007
This is a PDF file of an unedited manuscript that has been accepted for publication.
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http://dx.doi.org/doi:10.1016/j.enzmictec.2014.07.007http://dx.doi.org/10.1016/j.enzmictec.2014.07.007http://dx.doi.org/10.1016/j.enzmictec.2014.07.007http://dx.doi.org/doi:10.1016/j.enzmictec.2014.07.0078/11/2019 Morant 2014
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ISOLATION AND BIOELECTROCHEMICAL CHARACTERIZATION OF1
NOVEL FUNGAL SOURCES WITH OXIDASIC ACTIVITY APPLIED IN-SITU2
FOR THE CATHODIC OXYGEN REDUCTION IN MICROBIAL FUEL3
CELLS.4
Kyriale Vasconcelos Morant, Paulo Henrique da Silva, Galba Maria de Campos-5
Takaki and *Camilo Enrique La Rotta Hernndez.6
NPCIAMB - Ncleo de Pesquisas em Cincias Ambientais e Biotecnologia Centro de7
Cincias e Tecnologia (CCT) - Universidade Catlica de Pernambuco UNICAP,8
Recife PE, Brasil. Rua Nunes Machado, 42, Bloco J, Trreo, Boa Vista, 50050-590,9
Recife Brasil. Phone: +55 (81) 9927161210
*Corresponding author: [email protected]
ABSTRACT:12
Brazilian filamentous fungi Rhizopus sp. (SIS-31), Aspergillus sp. (SIS-18) and13
Penicillium sp. (SIS-21), sources of oxidases were isolated from Caatingas soils and14
applied during the in-situ cathodic oxygen reduction in fuel cells. All strains were15
cultivated in submerged cultures using and optimized saline medium enriched with 10 g16
L-1
of glucose, 3.0 g L-1
of peptone and 0.0005 g L-1
of CuSO4 as enzyme inducer.17
Parameters of oxidase activity, glucose consumption and microbial growth were18
evaluated. In-cell experiments evaluated by chronoamperometry were performed and19
two different electrode compositions were also compared. Maxima current densities of20
125.7, 98.7 and 11.5 A cm-2were observed before 24 h and coulombic efficiencies of21
56.5, 46.5 and 23.8% were obtained for SIS 31, SIS 21 and SIS 18, respectively.22
Conversely, maxima power outputs of 328.73, 288.80 and 197.77 mW m-3
, were23
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observed for SIS 18, SIS 21 and SIS31, respectively. This work provide the primary24
experimental evidences that fungi isolated from the Caatinga region in Brazil can serve25
as efficient biocatalysts during the oxygen reduction in air-cathodes to improve26
electricity generation in MFCs.27
28
Keywords: Oxidases,Filamentous fungi, Biocathodes, Biofuel cells, Cathodic Oxygen29
reduction.30
1. INTRODUCTION31
The gradual depletion of fossil fuels and the environmental concerns for their32
consumption have driven an intensive search for alternative sources for energy33
production. BioFuel Cells (BFC) are considered a promising alternative for clean energy34
generation and also obey general sustainability requirements (Karatay and Donmez,35
2011). However, the high cost of noble metals such as Au, Pt, Rh and Os, commonly36
used in coated electrodes as catalysts is still considered one of the limiting factors for37
scaled-up applications of microbial fuel cells (MFC) and conventional fuel cells. Even38
though, abiotic cathodes that use oxygen as electron acceptor are frequently adopted for39
BFC (Logan et al., 2006; Luo et al., 2010). Enzymes as biocathodes can potentially40
eliminate limiting factors such as: decreased efficiency due to the accumulation of41
metabolites, work under mild reaction condition such as temperature and pressure.42
Additionally, due to their high substrate specificity they are able to perform the electron43
transfer throughout suitable mediated systems and employing co-substrates (Da Silva et44
al., 2014; Farneth and DAmore, 2005). These types of enzymatic cathodes have been45
investigated in small scale enzymatic biofuel cells (Farneth and DAmore, 2005). On46
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the other hand, energy production obtained from the BFC is not yet satisfactory and47
their performance and power output generation can be affected by a number of factors,48
such as cellular activity, substrate biotransformation and the inefficient electron transfer49
from the biocatalysts to the electrodic materials. Studies on enzymes for electron50
interactions are being mainly focused on copper-containing oxidoreductases (Figure 1),51
which can catalyze the direct reduction of oxygen while perform the simultaneous52
oxidation of many organic compounds such as phenols. Mono and poly-phenol oxidases53
from fungal species such as:Agaricus bisporus (Shervedani and Amini, 2012), Coriolus54
hirsutus (Farneth and DAmore, 2005), Trametes versicolor (Lou et al., 2010)55
Coriolopsis gallica(Tinoco et al., 2001) and Pleurotus ostreatus(Barton et al., 2002);56
plant laccase from Rhus vernicifera; and bacterial laccase from Streptomyces57
coelicolor, were already studied and applied to these bioelectrodes (Shleev et al.,58
2005). Others less electrochemically explored, but highly promising corresponds to the59
fungal bilirubin oxidase (BOD) from Myrothecium verrucaria (Ivnitski et al. 2008;60
Mano et al., 2002) and bacterial BOD fromBacillus pumilus (Durand et al. 2012).61
EC 1.10.3.1 : Tyrosinase: polyphenol oxidase:62
2 catechol+O22 1,2-benzoquinone+2 H2O Eq. 163
EC 1.10.3.1: Laccase : Urishinol Oxidase64
4 benzenediol+O24 benzosemiquinone+2 H2O Eq. 265
EC 1.3.3.5: Bilirubin oxidase66
2 bilirubin +O22 biliverdin +2 H2O Eq.367
68
Laccase (LAC) and tyrosinase (TYR) are able to oxidize phenolic compounds and to69
reduce simultaneously oxygen into water (Eq. 1 and 2). Depending the microbial70
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source from which these enzyme were extracted, the redox potential of the T1site, may71
vary from 430 mV up to 780 mV vs.NHE (Palmore and Kim, 1999). Laccase from72
Trametes versicolor is the most attractive one since redox potential of its T1 site is73
ca.780 mVvs.NHE (Shleev et al., 2005). Nowadays, the best performances with laccase74
electrodes are obtained with osmium based polymers as redox mediators (Mano et al.,75
2002) Actually these electrodes are able to deliver a current density of 860 A cm-2
at76
only -70 mVvs. O2/H2O at pH 5.0. Under the same conditions, an identical current77
density is obtained at -400 mVvs.O2/H2O with a platinum wire as catalyst.78
Nevertheless, performances of laccase from Pleurotus Ostreatus electrodes drop79
drastically in the presence of chloride ions what constitutes both a major problem and a80
great challenge for its use in biofuel cells (Barton et al., 2002). On the other hand, BOD81
(Eq. 3) is naturally capable of catalyzing the oxidation of bilirubin into biliverdin and to82
simultaneously reduce dioxygen (Li et al., 2004). BOD is very similar to laccase. BOD83
electrodes are greatly related to the amino-acids sequence around T1 site of the enzyme84
(Shimizu et al. 1999). It is clearly reported that the most efficient BOD enzyme comes85
from Myrothecium verrucaria. Redox potential of its T1 site is included between 65086
and 750 mV vs. NHE, and its future application in BFC its close related with the87
observed thermal stability up to 60 C (Mano et al., 2002). These biocatalysts have88
been extensively used in cathodes for enzymatic fuel cells and electrochemical89
biosensors due to their high redox potential, however the almost mandatory use of90
electron shuttles such as 2,2 -Azino-bis(3-ethylbenzthiazoline-6-sulfonic acid) (ABTS)91
and other suitable molecules more recently studied as triphenylmethane dyes has been92
widely recognized as an effective way to avoid the loss of current during the93
bioelectrochemical process (Bach et al., 2013; Smolander et al. 2008; La Rotta et al.,94
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2011). However, the application of such enzymatic fuel bioelectrodes has been limited,95
specially attributed to the high costs of production and purification and the short half-96
life time associated with the enzyme inactivation in non-biological environments as the97
ones commonly found in the surface of electrodic materials of BFC. In this regard,98
biocathodes inoculated with the fungi for the in-situoxidase production may offer a99
potential solution (Wu et al., 2012; Rachinski et al., 2010). Also the in- situsecretion100
of oxidases by the filamentous fungi in air cathodes might be a more attractive way to101
achieve sustainable and cost-efficient electricity generation, especially for three main102
reasons: longer life-time of the biocatalysts since these are being produced under more103
compatible biological conditions; the use of low cost substrates such as residua or104
contaminated effluents; and the possibility of concomitant production of other natural105
occurring electro active molecules as microbial by-products like: azaphylones, quinone-106
like pigments as melanins, terpene as carotenoids, etc. The simultaneous utilization of107
such molecules could improve even more the couloumbic efficiencies by reducing the108
charge and mass transportation problems previously observed for these systems.109
PLEASE INSERTT FIGURE 1 HERE110
Currently, the Brazilian North and Northeast Network of Filamentous Fungi111
(RENNORFUN) aims to describe the biodiversity of filamentous fungi in soils from112
the Caatinga and the Amazon regions of Brazil throughout poly-phasic and molecular113
taxonomy as well as to demonstrate the applicability in industrial processes of the114
isolated micro-organisms and their by-products. In this context, this study aimed the115
isolation and identification of novel fungal species capable to produce biocatalysts with116
high oxidasic activity that can be applied to the cathodic reduction of oxygen in117
electrodes for biosensors and BFCs.118
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119
120
2. METODOLOGY121
2.1. Fungal Strains, media and cultivation conditions122
All strains belong to the RENNORFUN Culture Collection from the Catholic University123
of Pernambuco Brazil, stocked in slant tubes containing Sabouraud agar solid medium124
under refrigeration at 4o
C until their use. Initial selection was based on previous in-125
plate observations associated with pigment production and oxidase or tannase activities,126
since pigment production can be by-products of the reactions catalyzed by these127
enzymes (Koroljova-Skorobogat'ko et al., 1998; Saparrat et al., 2002). Table 1.Shows128
the culture media used for selection of fungal strains with oxidasic activity. Twelve129
fungal strains were originally chosen: two Rhizopus spp.; threeAspergillus spp.; three130
Penicillium spp.; twoEupenicillium spp and two Talaromycesspp. The microorganisms131
were visual evaluated in terms of substrate degradation and color formation, by132
cultivation in solid plates incubated for 48 at 28o C. For submerge cultures, a pre-133
inoculum of young mycelium disks of 0.8 cm of diameter were obtained from 2 days-134
old colonies in solid medium. Disks were disrupted in tubes and mycelium was re-135
suspended in fresh medium and incubated at 28o
C and 180 rpm for 48 hours. After this136
period of time, tubes were used for the inoculation of flasks containing 150 to 200 mL137
or microbial cathodic compartiments of 100 mL of capacity at the bicompartmented138
BFC. All cultures were incubated under the same controlled lab conditions.139
140
2.2. Microbial growth parameters and sample post-treatment141
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Comparisons between media composition and the effect over microbial parameters of:142
oxidase enzyme activity, final biomass (dried weight) and substrate consumption were143
performed. First, samples and culture brothswere separated from mycelia by filtration144
through nylon cloth and centrifugation at 4500 rpm for 20 minutes at 4o C. Mycelia145
were dried on paper filters at 60o C until constant weight. Finally, cell free supernatants146
were used for the quantification of glycerol or glucose using specific enzymatic kits147
purchased from BIOCLIN. Enzyme activities were determined using the below148
described methodologies.149
150
2.3. Oxidasic activity assays151
Enzymatic crude extracts and fermentation samples were evaluated in terms of oxidase152
activity using the methods summarized in Table 2. Oxidase and peroxidase activities153
were distinguished throughout similar methods; however for peroxidase activity 5.0154
mmol L-1
hydrogen peroxide was added instead a saturated oxygen buffer solution as155
oxidizing agent (assays 1 and 5, respectively). Mono and polyphenol oxidases were156
differentiated using assays 2 and 3 both in saturated oxygen buffer solutions. And157
finally the routine assay 4 was used for oxidase activity. All enzyme activities were158
expressed as international units per mL (UI mL-1
), defined as the amount of enzyme159
required to produce 1 mol mL-1 of the specific oxidized product, according to the160
specific molar extinction coefficients, per minute under the reaction conditions used in161
each assay. The increase in absorbance was monitored in a UV-Vis spectrophotometer162
BioChrome Libra S32 .163
PLEASE INSERT TABLE 1 HERE164
PLEASE INSERT TABLE 2 HERE165
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2.4. Electrochemical analyses166
Chronoamperometric analysis:A bicompartmented BFC was employed (Scheme 1). A167
100 mL cathodic compartment was composed by the fungal culture using the selected168
medium, and two electrodic materials were evaluated. Immersed carbon felt electrodes169
coated with carbon Black Vulcan plus 0.5% Pt (w\w) in PTFE or a Pt-free Black170
Vulcan coated carbon felts; As anodes, immersed plates of exploded graphite in 20171
mmol L-1
potassium ferrocyanide were used. All electrodes had 19.6 cm-2
of surface172
area. As cation exchange system a saline bridge of agar in saturated KCl was used. The173
potential (E) vs. time (min) was recorded using a multimeter Fluke 8080 with data174
acquisition software. All experiments were allowed to stabilize for about 30 minutes175
before each measurement. Chronovoltammetric data were converted into Iddata using176
the Ohms Law expression (Equation 4) since an external load resistance of 1 K was177
employed.178
Id= E * R Eq. 4179
The Coulombic efficiency (%) in Equation 5, was calculated from the following180
expressions according to previous studies (Logan et al., 2006; Dantas et al., 2013).181
CE= (CR/CT) Eq. 5182
where, CTcorresponds to the theoretical amount to be obtained from each substrate and183
CR corresponds to the practical coulombs recovery from the substrate. CT can be184
calculated at any time using the expression:185
CT = nzF Eq. 6186
wherenis the moles of substrate, zare the moles of electrons per mol of substrate (O2=187
4e-, Glucose = 6 e
-or Glycerol= 12 e
-); and F is the Faradays constant 96485.4 C188
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mol-1. Applying Equation 6 to an integrated model of Id vs time for a microbial fuel189
cell we obtain Equation 7190
CE= M / F z VAC/CC S Eq. 7191
where M is the substrate molarity, A the electrode surface area, V is the total volume192
circulated inside the cathodic compartment and Sis the final substrate concentration.193
PLEASE INSERT SCHEME 1 HERE194
Cyclicvoltammetric analysis: The electrochemical system was composed by a glass 15195
mL glass cell, a 0.5 cm diameter glassy carbon as working electrode, a Pt wire of 1.0 cm196
as counter-electrode and Ag|AgCl2in saturated KCl as reference electrode. As enzyme197
substrate 1.0 mmol L-1
pyrogallol was used. And as support electrolyte 100 mmol L-1
198
Sodium acetate buffer solution pH 5.0 was employed. The cell was coupled to a199
PalmSens potentiostat/galvanostat with data acquisition software PS-Trace 4.4.200
Cyclic voltammetry parameters included: Pre-treatment of -1.2 V, 10 s; E deposition: -201
1.0 V, 10 s; T eq.: 8 s; E start: 0 V; E vertex 1: -0.2 V; E vertex 2: 1.0 V; E step: 0.005202
V and Scan rate: 0.05 V s-1
. All readings used at least 5 scans.203
204
Polarization analysis and power output determination: Using the same electrochemical205
system for the MFC, but placing the reference electrode at the cathodic compartment206
and same apparatus described above, samples with the highest recorded activity were207
analyzed in terms of cathodic current densities within potential range of: 0.80 to -0.5 V.208
The following parameters were used: OCV of 0.85 V vs Ag|AgCl in sat. KCl; Linear209
sweep: 8 s, Eo = 0.8 V, Ef =-0.5 V, Estep= 0.002 V, Scan rate 0.01 V s-1
. The polarization210
curves of Id vs E obtained were used to the determination of the Power-output curves (Pd211
vs E) and maxima Pdvalues according to Equation 8212
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Pd= E * Id Eq. 8213
214
215
3. RESULTS AND DISCUSSION216
3.1. Screening of novel fungal oxidases217
Initially the solid culture medium A (MA) was supplemented with gallic acid or tannic218
acid as carbon sources, to visualize the production of oxidase or tannase in plates by the219
formation of green to black halos according to previous studies (Leite et al., 2012;220
Koroljova-Skorobogat'ko et al., 1998; Saparrat et al., 2002). Results from the screening221
in MA supplemented with those substrates can be observed in Table 3. Six of twelve222
strains presented the availability to degrade tannic acid and only four were able to223
oxidize efficiently gallic acid. Unexpectedly, only one strain (SIS-21) showed both224
pigments production and exhibited high oxidase and tannase activities, while the other225
pigment producers strains showed low to moderate tannase activity and none oxidase226
activity. Since one of the goals of this study was also to find fungal strains able to227
biotransform alternative carbon sources, different than glucose (Ex. Glycerol), with the228
retention of the oxidasic activity, the use of a modified medium A or (MMA), enriched229
with glycerol was also tested. Nevertheless, only strains SIS-18, 21, 31 and 39 retained230
the availability of performing the oxidization of gallic acid in plates while grew very231
well in a medium containing glycerol.232
PLEASE INSERT TABLE 3 HERE233
This also was confirmed when the pre-selected strains according to the halo formation234
in plates containing (MA) and (MMA) media, were cultivated in liquid medium (B) or235
modified medium B (MMB) where glycerol was added instead glucose as can be seen in236
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Table 4. As such, no oxidase activity was observed at all in MMB. At this point the best237
oxidase producers corresponded to strains SIS-21, 31 and 18, with 5, 1.7 and 1.6 KU238
mL-1, respectively. For the next experiments only these three strains were evaluated.239
Finally, since the presence of copper was already mentioned as a beneficial inducer of240
oxidase enzymes as blue-oxidases (Ex. LAC, TYR and BOD) (Fonseca et al., 2010),241
this was added to the medium B (MB), now called Copper-medium B or (CuB). As it242
was expected a significant increase on oxidase activity was observed in all cases. This243
increase represents almost 1.65 fold-times in the case of the oxidasic activities observed244
for SIS 18 and SIS-21, an almost 2.4 fold-times in the case of SIS-31. In contrast, SIS245
21 showed the highest values for fungal growth in terms of dried weight of 1.02 g, and246
lower fungal growths were observed for SIS 31 followed by SIS 18, with 0.43 and 0.95247
g, respectively. In terms of glucose consumption, all three strains caused the complete248
depletion of this substrate in 120 h.249
PLEASE INSERT TABLE 4 HERE250
Since the oxidation of pyrogallol can be unspecific in terms of which oxidasic activity is251
present in the fungal cultures, specific assays were performed using cell free samples252
obtained from submerged cultures in CuB medium, in a way to identify which one of253
the oxidase activities (monophenol oxidase - LAC, polyphenol oxidase -TYR or254
bilirubin oxidase - BOD) or eventually if peroxidase activity (POD) was present. Table255
5 shows this activity characterization performed for the three selected fungal strains.256
Thus, as clearly appeared, none of the evaluated strains showed any POD activity, since257
no oxidation products were observed in the absence of oxygen and the presence of258
hydrogen peroxide. Likewise, when BOD was evaluated using bilirubin as specific259
substrate in the presence of oxygen, no oxidized products were observed either. On the260
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other hand, when samples were tested in terms of oxidase activity using specific261
substrates in the presence of oxygen, interesting results were found. Firstly, only two262
strains presented LAC activity, corresponding toPenicilliumsp. (SIS-18) andRhizopus263
sp (SIS-31). Additionally, both fungi showed almost half of the oxidase activity264
observed when the unspecific assay of pyrogallol was used. At that point, when TYR265
activity was tested only Aspergilllus sp. and Rhizopus sp. showed a fraction of the266
observed activity with the unspecific assay. These discrepancies among oxidase267
activities can be related with the specificity that each enzyme has for each substrate268
used during the assays. According to the available enzyme data bases, no records269
relating mono or polyphenol oxidases have been yet found for Rhizopus sp, but270
polyphenol oxidases was already reported for two Aspergillusspp.: A. niger (Sutay et271
al., 2008) andA. oryzae (Gasparetti et al., 2009); On the other hand, several laccase-like272
enzymes were already reported for several Penicillium spp., such as P. acuelatum, P.273
cyclopium and P. digitatum (El-Shora et al., 2008). These results are very promising274
since a novel fungal species asRhizopusis now being discovered as source of not one,275
but two different oxidase activities.276
PLEASE INSERT TABLE 5 HERE277
3.2. Electrochemical studies278
Fig 2. shows the cyclic voltammograms (CV) obtained for cell free culture media279
samples containing the highest oxidasic activity observed for the selected fungi. At280
first, it can be observed that profiles showed to be very similar for all strains, but281
slightly higher cathodic currents were observed for SIS 18 and 31. Also a wide282
reduction peak, probably corresponding to a process of two close reduction events was283
observed for SIS-31 between 500 and 800 mV. On the other hand, a higher redox span284
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can be expected for Tyrosinase, since not one but two oxidations can occur over the285
same molecule, or one -OH insertion on a phenolic ring following by a dual oxidation286
process causing the formation of quinone-like derivatives (La Rotta et al., 2011).287
Monophenol oxidase activity observed for SIS-21 and its voltammetric profile was in288
accordance to previous studies where, a lower redox span was observed for LAC289
(Fernndez-Snchez et al., 2002). In general, control experiments with all enzymatic290
extracts in the absence of substrate confirmed the enzymatic oxygen reduction, but in all291
cases low electrochemical activity ranging only 2 to 4 A, were observed.292
PLEASE INSERT FIGURE 2 HERE293
When CVs were repeated in the presence of the unspecific substrate pyrogallol, more294
asymmetric anodic and cathodic peak shapes were detected in potentials ranging295
between -0.2 to 1.0 V vs. Ag|AgCl sat. KCl. This response was especially evident in the296
case of SIS 21 between 0.6 and 0.8 V, where an increase on anodic current of 10 A,297
was achieved. The same response was observed for the other two strains but at lower298
levels, being only of 7 A and 3 A for SIS-31 and SIS-18, respectively. The299
substantial shift of currents demonstrates the active catalysis of the enzymatic oxygen300
reduction at the surface of the working electrode, and the simultaneous oxidation of the301
substrate, indicating that an active oxidase was being detected in all cases. Since most of302
oxidase enzymes are multicenter enzymes, intermediate redox states are expected. We303
assume that the pair of anodic and cathodic redox peaks in the evaluated samples can be304
attributed to the process of direct electrical transfer between the T2/T3 redox copper305
center of the oxidase and the glassy carbon electrode, being mediated by the oxidized306
forms of pyrogallol. Also, oxidation of the pyrogallol can easily occur on any of the 307
OH groups, and its hardly expected to occur a simultaneous oxygen insertion.308
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Pyrogallol oxidation is mostly followed by the formation of a cycled oxidized derivative309
called purpurogallin. Finally, voltammetries were repeated in the presence of a specific310
substrate for TYR or poly-phenoloxidase. Cresol corresponds to a methyl derivative of311
phenol, that can be easily oxidized to quinone by the insertion of an oxygen atom312
depending on the activation caused by the -CH3 position respect the OH group. As313
such, this substrate can be oxidized not once but twice, and under strong oxidizing314
conditions cycled derivatives are not formed, instead of them poly-quinone-like315
derivatives can be appeared as dark precipitates since they are usually insoluble in water316
(Ramsden and Riley, 2014). As we expected, the results pointed the main polyphenol317
oxidase to be present in SIS-31, confirming our previous biochemical observations.318
Clearly, SIS-31 possess a strong oxidation peak of 4 A was observed at 100 mV,319
followed by a 2 A reduction peak at 200 mV. Similar, but lower currents of Ia= 2 A320
and Ic = 1 A, were observed at the same potentials for SIS-18. In contrast, no321
significant response was observed for SIS-21, confirming the absence of tyrosinase322
activity for this strain. The chronoamperometric analyses were used to determine323
electrochemical parameters of maxima current intensities during the cultivation and in-324
situ simultaneous oxygen reduction. These profiles allow us to determine the amount of325
electrons that effectively were starved from the substrate, and expressed them as326
coulombic efficiencies. The profiles obtained for the evaluated fungal strains cultivated327
at air-cathodes using medium CuB , during 120 h can be observed in Fig. 3. Since no328
significant changes in current densities were observed from the 72 h up to end of the329
experiment at 120 h, only these data are shown. In-situ culture experiments were330
compared with the response of a simulated behavior observed for the addition of 900 UI331
mL-1
of Laccase from Trametes versicolor (LAC Tv) to a volume of 100 mL of fresh332
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CuB medium. The chronoamperometric profile for control LAC Tv was very flat333
compared with the highest density current peaks observed when all three strains334
evaluated in-situ.335
PLEASE INSERT FIGURE 3 HERE336
The summarized results achieved with the chronoamperometries are shown in Table 6.337
Maximum current densities were observed for SIS 31 followed by SIS 21 and SIS 18,338
with 125.75, 98.68 and 29.75 mA cm-2, respectively. While for the experiment339
containing pure LAC Tv the lowest value of 11.47 mA cm-2, -was observed. Even when340
we tried to mimic the same conditions present during the fermentations, including341
enzyme concentration, many factors could affect the activity of pure LAC Tv causing342
such low response, including: enzyme inactivation, electrode deposition and passivation343
or lack of a suitable electron transfer mechanism, that can be present while the fungi are344
growing. These observations are in concordance with previous studies about MFC345
using fungus-based biocathodes, where longer and stable performances were achieved346
for the fungal cultures than with the pure laccase-based controls (Wu et al., 2012).347
Moreover, the fungi inoculated into the MFC had about 12-time higher current densities348
(in the case of SIS 31) than the control using carbon electrode and free LAC from349
Trametes versicolor. This clearly shows that the oxygen reduction in the air biocathodes350
can be efficiently performed and enhanced by the used of in-situ fungal cultures. For the351
coulumbic efficiency, it was observed that all strains have, from moderate to very good352
levels of electron starvation from the substrate (in terms of glucose biotransformation).353
Especially, SIS-31 achieved a very high value of CEof 56.5%, which means that this354
fungus is able to remove almost 50% of the electrons available in the substrate to the355
biocatalyst during its biosynthesis and reducing the available oxygen present inside the356
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media. Good results of 46.5 and 23.8%, were also achieved for SIS-21 and SIS-18,357
respectively. Even when SIS-21 produced almost 2 fold-times more biomass than SIS-358
31 and achieved the maximum unspecific oxidase activity of 5000 UI mL-1 among the359
evaluated strains, only SIS-31 was more efficient transforming the substrate during the360
fermentation into tyrosinase and laccase and subsequently this conducted to a higher361
and more stable production of energy in-situ.362
PLEASE INSERT TABLE 6 HERE363
The power outputs observed for the strains and the enzyme control of LAC-Tv were364
compared using two different electrode compositions. At first, all experiments were365
evaluated with free-platinum carbon air cathodes. As such, Figure 4, exemplifies the366
polarization curves and power output profiles that were obtained for this approach. The367
highest power outs were observed for SIS-18 and SIS-21, with close values of 328 and368
288 mW m-3
, respectively. In contrast, with previous observations, SIS-31 showed only369
197 mW m-3, being the lowest value among strains. This could indicate that even when370
this microorganism starves efficiently electrons from the substrates, the produced371
enzyme did not perform very well the cathodic oxygen reduction or that some372
unidentified problems related with charge or mass transportations were present. The373
control experiment using LAC Tv showed the lowest value of 43.4 mW m-3
. This374
proved again that the fungal metabolites present inside the cultures and the crude375
extracts contributed indeed to improve the energy generation inside the biocathodes.376
Since similar enzyme concentrations were used, this cannot be consider as the direct377
responsible for the power loss.378
PLEASE INSERT FIGURE 4 HERE379
PLEASE INSERT FIGURE 5 HERE380
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The second electrode approach used a Pt load of 0.5% (w/w), and intended to identify if381
a real improvement can be achieved in electrodes with no metallic catalysts and with the382
addition of fungal oxidases. These results were put together in figure 5. Using as383
control experiment a submerge electrode in free-enzyme medium, a very low level of384
cathodic oxygen reduction of just 5.46 mW m-3 was observed. When the electrode385
contained Pt, an increase of almost 75 mW m-3
was observed. Similar increases were386
observed in all cases, following the same patter observed for Free-Pt electrodes. As387
such, were observed increases of 100, 60 and 20 mW m-3, when we used crude extracts388
of SIS-18, SIS-21 and SIS-31, respectively. Comparing both systems it can be observed389
that the differences are not quite significant between an oxidase biocathode plus free-pt390
electrode and when the Pt-loaded electrode was used. These differences were really391
evident when no catalysts were used and between pure enzyme electrodes and the ones392
obtained by in-situ cultures.393
394
4. CONCLUSIONS395
Three strains were selected as the best producers of oxidasic activity and then can be396
used as potential biocatalysts for oxygen reduction in MFCs air-cathodes. The efficient397
utilization and biotransformation of glucose was observed specially for Aspergillus sp398
SIS 18. and Rhizopus sp. SIS 31. However, all strains showed low oxidasic activity in399
the presence of glycerol; Penicillium sp. - SIS 21 was responsible for the highest400
generation of current density, while SIS 31 showed the best transformation of glucose401
into energy according to the highest coulombic efficiency observed. This fact, turn the402
oxidases from these microorganisms into potential targets for the isolation,403
characterization and use of their biocatalysts applied to the oxygen reduction in biotic404
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cathodes. The results thus far suggest the observed electrochemical activity is due to the405
oxidase enzymes. This family of enzymes can catalyze the four-electron reduction of406
O2to H2O coupled to the one-electron oxidation of different substrates. In nature these407
electrons are supplied by several phenols, amines, and lignins, as well as inorganic ions.408
Thus, the production of these biocatalysts in air-cathodes for MFC can be also coupled409
to the degradation of some interesting substrates including pollutants as phenolic410
compounds and dyes present in waste-waters. In a MFC, electrons were replenished to411
the cathode from the anode, which accepts electrons from anode-respiring and other412
bioentities with cross-membrane electron transfer capabilities. The results above413
provide the primary experimental evidences that fungi isolated from the Caatinga region414
in Brazil can serve as efficient biocatalysts during the oxygen reduction in air-cathodes415
to improve electricity generation in MFCs. Such biosystem confers many advantages416
over conventional abiotic or pure enzyme cathodes, such as low costs, good pH417
buffering capability and the possibility for sustainable MFC operation.418
419
Acknowledgments420
The authors wish to thank the Regional Scientific Development Research Grant421
Program (DCR No.0008-1.06/11) and Scientific Initiation Grant Program given by the422
Brazilian Research Council - CNPq and The Foundation for Support of Science and423
Technology from the State of Pernambuco - FACEPE, Brazil. Special thanks are given424
to the NPCIAMB from the Catholic University of Pernambuco for the facilities and425
infrastructure used during the execution of this research. And the invaluable help given426
by the group of Electrochemistry from the Institute of Chemistry University of So427
Paulo, Brazil.428
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429
430
REFERENCES431
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characterization, and identification of a novel bifunctional catalase-phenol oxidase from521
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34. Wu, C.; Liu, X.W., Li, W.W.; Sheng, G.P.; Zang, G.L.; Cheng, Y.Y.; Shen, N.; Yang, Y.P.;525
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6418-6424.530
531
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532
533
534
535
Anode
Air Cathode
Saline bridge
Fungal mycelium
V
50 mm
Cathodic
compartment
Anodic
compartment
Air
Inlet
Fe +2| Fe +3
Enzyme Ox
Enzyme Red
H2O
O2 + H+
e-
e-
536
Scheme 1. Diagram for the bicompartmented microbial fuel cell using an air-cathode537
and in-situ fungal growth.538
539
540
541
542
543
544
545
546
547
548
549
550
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551
552
553
554
Table 1.Culture media used for screening of fungal strains with oxidasic activity.555
Solid Media Liquid Media
MA* MA MMA MB [27,28] MMB [27,28] CuB
Component / g L-1 Component / g L-1
Peptone
Meat ext.
Tannic acid
Agar
6.0
4.0
4.0
4.0
Peptone
Meat ext.
Gallic acid
Agar
6.0
4.0
5.0
4.0
Glycerol
Peptone
Meat ext.
Gallic acid
Agar
20.0
6.0
4.0
5.0
4.0
Glucose
Peptone
KH2PO4
ZnSO4
K2HPO4
FeSO4
MnSO4
MgSO4
10.0
3.0
0.6
0.001
0.4
0.0005
0.05
0.05
Glycerol
Peptone
KH2PO4
ZnSO4
K2HPO4
FeSO4
MnSO4
MgSO4
20.0
3.0
0.6
0.001
0.4
0.0005
0.05
0.05
Glucose
Peptone
KH2PO4
ZnSO4
K2HPO4
FeSO4
MnSO4
MgSO4
CuSO4
10.0
3.0
0.6
0.001
0.4
0.0005
0.05
0.05
0.0005
*Media used for visualization of tannase activity in plates.556
557
558
559
560
561
562
563
564
565
566
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567
568
569
570
Table 2.Enzyme activity methods used for screening of oxidasic enzymes.571
Enzyme
Activity
for:
Substrate
Initial
concentration
Co-
substrate
Buffer, pH,
Temperature
Product | ABS Ref.
Oxidase Pyrogallol | 0.01
mmol L-1
O2 100 mmol L-1
Acetate Buffer pH
5.0 at 25
o
C
Purpurogallyn |
24,700 mol L1cm
1
at 420 nm
(Xican, 2012;
Ghadiri et al., 2013)
Laccase Syringaldazine |
0.05 mmol L-1
O2 20 mmol L-1
Phosphate buffer,
pH 7.0 at 30C
Oxidized Syringaldazine
|
65,000 mol L1cm1
at 525 nm
(Harkin and Obst, 1973;
;Espin et al., 1998)
Tyrosinase 3-Methyl-2-
benzothiazolinone
hydrazone | 6.0
mmol L-1
O2 20 mmol L-1
Phosphate buffer,
pH 7.0 at 30C
L-DOPA |
38,000 mol L1cm
1
at 505 nm
(Harkin and Obst, 1973;
Espin et al., 1998)
BOD Bilirubin | 0.002%
(w/v)
O2 200 mmol L-1Tris
HCl buffer, pH 8.4
at 37C
Biliverdin |
56,300 mol L1cm
1
at 440 nm
(Kimura et al., 1999)
Peroxidase Pyrogallol | 0.01
mmol L-1
Syringaldazine |
0.05 mmol L-1
H2O2
H2O2
100 mmol L-1
Acetate Buffer pH
5.0 at 25oC
20 mmol L-1
Phosphate buffer,
pH 7.0 at 30C
Purpurogallyn |
24,700 mol L1cm
1
at 420 nm
Oxidized Syringaldazine
|
65,000 mol L1cm1
at 525 nm
(Xican, 2012; Ghadiri
et al., 2013)
(Harkin and Obst, 1973;
Espin et al., 1998)
572
573
574
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575
576
Table 3. Preliminary selection of fungal strains with oxidase activity and pigment577
production based on observations made in plates.578
RENNORFUN
CODE
Microorganism
Pigment
production
Tannase assay Oxidase
Assay
SIS-39 Rhizopus sp. - ++ ++
SIS-31 Rhizopus sp. - +++ +++
SIS-18 Aspergillus sp. - +++ ++
SIS-27 Penicillium sp. - +++ +
SIS-4(E) Aspergillus sp. Red ++ -
SIS-7 Aspergillus sp. Dark + ++ -
SIS-21 Penicillium sp. Yellow ++ +++ +++
CP1 10-3 H Penicillium sp. Green ++ ++ -
N.C. Eupenicillium sp. Orange ++ - -
A2P1 10-3 Eupenicillium sp. Orange + - -
A2P1 10-4 G Talaromyces sp. Orange ++ + -
A2P1 10-3 Talaromyces sp. Orange + - -
NC = Not codified.579
Intensity of color = Negative or absence (-); Positive weak (+); Positive moderate (++); Positive strong (+++)580
581
582
583
584
585
586
587
588
589
590
591
592
593
594
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614
615
Table 5.Analyses for oxidasic activity present in the crude extracts.616
Strain Oxidase Activity Tested( UI mL-1)
Unespecific
Phenol Oxidase
Activity
Assay 1
Monophenol
oxidase Activity
LAC
Assay 2
Polypheno
oxidasel Activity
TYR
Assay 3
Bilirubin
oxidase Activity
BOD
Assay 4
Peroxidase
Activity
POD
Assay 5
Aspergillussp. SIS
18
2630 131.5
N.R 1200 60.0 N.R. N.R.
Penicillium sp.SIS
21
8900 445.05600 280.0 N.R. N.R. N.R.
Rhizopus sp. SIS 31 4180 209.0 2580 129.0 1400 70.0 N.R. N.R.
N.R.: Negative or no response617
618
619
620
621
622
623
624
625
626
627
628
629
630
631
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632
Table 6. General results for the chronoamperometric analyses during in-cell633
experiments.634
635
636
637
638
639
640
641
642
Fungal Strain
Maximum Oxidase
Activity achieved in-situ
(UI mL-1) at 120h
Idmax
(
A cm-2)
Time of
Idmax
(h)
Residual
Glucose
(g L-1) at 120h
*CE
(%)
Aspergillussp. SIS 18 2800 140 29.75 1.0 13 0.000 0.0005 23.8 1.2
Penicillium sp. SIS 21 4600 230 98.68 1.0 23 0.001 0.0005 46.5 2.3
Rhizopus sp. SIS 31 2700 135 125.75 1.0 23 0.003 0.0095 56.5 2.8
Laccase from Trametes
versicolor 600 30 11.47 1.0 1 0.000 0.0005 --
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Laccase Tyrosinase
BOD
O2 H2O
O2 H2O
O2 H2O
643
Figure 1. Reactions catalyzed by multi-copper oxidases applied to biocathodes644
645
646
647
648
649
650
651
652
653
654
655
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-0.2 0.0 0.2 0.4 0.6 0.8 1.0-4
-2
0
2
4
6
8
10
12
I,A
E, V
Aspergillus sp. SIS-18
-0.2 0.0 0.2 0.4 0.6 0.8 1.0-4
-2
0
2
4
6
8
10
12
I,
A
E, V
Penicillium sp. SIS-21
-0.2 0.0 0.2 0.4 0.6 0.8 1.0-4
-2
0
2
4
6
8
10
12
I,A
E, V
Rhizopus sp. SIS-31
656
Fig. 2.Cyclic-voltammograms for the selected fungal strains. Control of 200 UI mL-1657
cell free sample (blue), plus 0.01 mol L-1 pyrogallol (red); plus 0.01 mol L-1 cresol658
(green); Potential was measured versus a Ag|AgCl in sat. KCl. Scan rate: 5 mV s-1
.659
660
661
662
663
664
665
666
667
668
669
670
671
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0 12 24 36 48 60 72
0
20
40
60
80
100
120
140Control Lac Tv
SIS 31
SIS 21
SIS 18
Id,mAc
m-2
Time, h
672
Fig. 3. Chronoamperometric profiles for the selected strains observed during 120 h at673
25oC in medium BCu compared to a control of free cell medium dopped with Lacase674
from T. versicolor.675
676
677
678
679
680
681
682
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-0.6
-0.4
-0.2
0.0
0.2
0.4
0.6
0 1 2 3 4 5 6
Id, A m-3
E,V
0 1 2 3 4 5 6
0
50
100
150
200
250
300
350
400SIS18
SIS21
SIS31
Pd,mWm
-3
I, A m-3
328.73
288.80
197.77
43.40
683
Figure 4.Power density output profiles obtained from the polarization curves (in-set684
plot) for crude extracts obtained from cultures of SIS-21 (black), SIS-18 (red) and SIS-685
31 (blue). And free cell medium doped with 900 UI of Lac Tv (green) was used as686
control.687
688
689
690
691
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Control LAC TV SIS 18 SIS 21 SIS 31
0
100
200
300
400
500
Pdmax,mWm
-3
75.80
5.46
105.46
43.40
438.16
328.73
344.10
288.90317.30
197.80
692
Figure 5. Maxima In-cell Power-outputs (vs Ag|AgCl2 sat. KCl) for crude extracts with693
the highest oxidasic activity obtained from the evaluated strains applied in to air694
biocathodes using two different electrode compositions: 0.5% (w/w) Pt-Black Carbon695
PTFE carbon felt (grey bars) and Free Pt Carbon PTFE carbon felt (white bars).696
Control experiments contain no enzyme.697
698
699
700
701
702
703
Highlights704
We isolated three novel filamentous fungi with high oxidasic activity from705
soils of the Brazilian Scrubland (Caatinga).706We found interesting mono- and poly-phenol oxidasic activities707
compared with other fungal sources.708
These fungal strains were applied during the in-situ cathodic reduction of709
oxygen in microbial fuel cells air-cathodes .710
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Accepte
dManu
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In bioelec trochemical terms, we observed high current densities and711
power out generations.712
Also high levels of substrate biotransformation into energy according to713
the coulombic efficiency were observed.714
715
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