Open Access

Whole resting cells vs. cell free extracts of Candida parapsilosis ATCC 7330 for the synthesis of gold nanoparticles

AMB Express20166:92

DOI: 10.1186/s13568-016-0268-y

Received: 15 August 2016

Accepted: 3 October 2016

Published: 7 October 2016

Abstract

The cell free extracts of Candida parapsilosis ATCC 7330 are more efficient than the whole resting cells of the yeast in the synthesis of directly usable gold nanoparticles as revealed by this systematic study. Cell free extracts yielded gold nanoparticles of hydrodynamic diameter (50–200 nm). In this study, the total protein concentration influences the nanofabrication and not only the reductase enzymes as originally thought. Powder X-ray diffraction studies confirm the crystalline nature of the gold nanoparticles. Fourier Transform Infra Red spectroscopy and thermal gravimetric analysis suggests that the biosynthesized gold nanoparticles are capped by peptides/proteins. Dispersion experiments indicate a stable dispersion of gold nanoparticles in pH 12 solutions which is also confirmed by electron microscopic analysis and validated using a surface plasmon resonance assay. The effectiveness of the dispersed nanoparticles for the reduction of 4-nitrophenol using sodium borohydride as a reductant further confirms the formation of functional gold nanoparticles. It is also reported that gold nanoparticles with mean particle diameter of 27 nm are biosynthesized inside the whole cell by transmission electron microscopy analysis. With optimized reaction conditions, maximum gold bioaccumulation with the 24 h culture age of the yeast with cellular uptake of ~1010 gold atoms at the single cell level is achieved but it is not easy to extract the gold nanoparticles from the whole resting cells.

Keywords

Candida parapsilosis ATCC 7330 Whole resting cells Cell free extract Culture age Gold nanoparticles Dispersion stability

Introduction

Microorganisms play a key role in the removal of toxic heavy metals and metalloids from the polluted environment by biosorption, bioaccumulation, biotransformation and biomineralization (Dixit et al. 2015; Gadd 2010; Reith et al. 2007). There is also an emphasis on using microbes for the synthesis of nanoparticles as compared to chemical methods since the microbe mediated methods are environmentally benign and sustainable (Sharma and Mudhoo 2010; Singh 2015; Virkutyte and Varma 2013). Among the microbes, fungi are well known for heavy metal binding, uptake and accumulation (Dighton and White 2005). Fungal species are efficient biological systems for the synthesis of metal nanoparticles (Boroumand Moghaddam et al. 2015). Among the noble metal nanoparticles, gold nanoparticles are widely used for diverse applications in diagnosis, therapy and catalysis (Eustis and El-Sayed 2006). Compared to bacteria, synthesis of gold nanoparticles using fungal systems has advantages such as the ease of handling/scale up, presence of redox enzymes and capping agents for enhanced productivity (Yadav et al. 2015). The initial report on fungus mediated preparation of gold nanoparticles used the Verticillium sp. where the nanoparticles are formed intracellularly (Mukherjee et al. 2001) but the isolation of nanoparticles from the cells is still quite a challenge.

Pichia jadinii (Gericke and Pinches 2006b) produces spherical gold nanoparticles intracellularly whereas Y. lipolytica (Agnihotri et al. 2009) biosynthesized nanoparticles remain associated with the cell wall. Besides spherical gold nanoparticles, yeast species are also reported to produce nanoparticles of varying size and morphology e.g. triangular and hexagonal gold nanostructures are produced with extracts of V. volvacea (Philip 2009). Using yeast species, formation of cadmium sulfide (Dameron et al. 1989), lead sulfide (Seshadri et al. 2011), titanium dioxide (Jha et al. 2009a) and antimony oxide (Jha et al. 2009b) nanoparticles are also reported.

Microbial production i.e., whole resting/fermenting cells, cell free extracts, isolated proteins and culture supernatants can be used for the production of nanoparticles. Whole intact cells which are harvested from the culture media are commonly referred to as resting cells and cell free extract is the crude fraction obtained after lysing the resting cells. Candida parapsilosis ATCC 7330 is reportedly an established biocatalyst for various organic biotransformations to produce optically pure secondary alcohols and amines (Mahajabeen and Chadha 2013; Venkataraman and Chadha 2015). It is also observed that the biocatalytic activity of this yeast is found to vary with the culture age used for the biotransformation (Kaliaperumal 2011). There are not too many detailed reports on the correlation between the microbial culture age and biogenesis of gold nanoparticles. The bacteria Thermus scotoductus SA-01 shows that the maximum removal of Au in the form of nanoparticles occurs during the late exponential phase (Erasmus et al. 2014). In a separate study, the synthesis of silver nanoparticles using the cell free filtrates obtained from 4 to 7 days culture of Penicillium nalgiovense AJ12 shows the importance of culture age (Wang and Chen 2009). Even though these reports have specified the importance of microbial culture age, the other parameters which affect the metal bioaccumulation are not dealt with. This study shows the optimization of parameters such as culture age, biomass concentration and incubation time for the biosynthesis of gold nanoparticles using the intact whole cells of Candida parapsilosis ATCC 7330 and the utility of the cell free extract prepared from the resting cells for the biosynthesis of gold nanoparticles. In addition, experiments to improve the monodispersity of particles formed by the yeast cell free extract is presented.

Materials and methods

General

Gold (III) chloride (99 % pure) and Bradford reagent were procured from Sigma Aldrich. Yeast malt broth media constituents (peptone, yeast extract, malt extract; dextrose) and phenyl methane sulfonyl fluoride (PMSF) were purchased from Hi Media laboratories. Buffering reagents such as potassium dihydrogen phosphate and dipotassium hydrogen phosphate were purchased from Merck. Enzyme cofactors such as Nicotinamide adenine dinucleotide (NADH) and Nicotinamide adenine dinucleotide phosphate (NAD(P)H) were procured from Sisco Research Laboratory chemicals. All set of experiments was performed using ultra pure MilliQ H2O (resistivity: 18.2 MΩ cm). All the reaction flasks were washed with aqua regia (3: 1 v/v of Conc. hydrochloric acid and nitric acid) before use.

Microorganism growth conditions and growth behavior in liquid medium

Candida parapsilosis ATCC 7330 strain was procured from ATCC, Manassas, VA 20108, USA and grown in yeast malt broth (YMB) media consisting of 5 g L−1 peptone, 3 g L−1 yeast extract, 3 g L−1 malt extract and 10 g L−1 dextrose. Yeast malt agar slant was prepared at monthly intervals to maintain stock culture under sterile conditions. For preculture, about two loops (4 mm diameter) was inoculated in sterilised 50 mL media and incubated in an orbital shaker at 200 rpm at 25 °C. For the main culture, about 4 % v/v of preculture was inoculated into sterilised 50 mL YMB broth medium and incubated for respective growth periods according to the aforementioned conditions. The yeast culture and preservation conditions were followed as per established procedures (Kaliaperumal et al. 2010). The growth behavior of Candida parapsilosis ATCC 7330 in liquid medium was studied by monitoring the optical density (OD600) and dry cell weight as a function of time. Samples were diluted for optical density measurements so as to keep the OD values lesser than 1.0.

Biosynthesis of gold nanoparticles using resting cells

Different culture ages of the yeast (24, 36 and 48 h) of 50 g L−1 concentration were used for the biosynthesis of gold nanoparticles. To the cell suspension prepared with phosphate buffer (pH 7.0, 20 mM), gold (III) chloride was added to make an overall concentration of 1 mM. The reaction flask was maintained at 37 °C, 200 rpm for 72 h. The amount of Au removal from the aqueous solution was determined for different culture ages. After 72 h reaction, the yeast cell suspension was removed from the reaction mixture and the remaining supernatant was used to estimate the amount of gold left over. Through mass balance calculations, the amount of gold loaded into the yeast cells was determined.

In order to determine the optimum cellular concentration, the biomass concentration was varied for the fixed metallic precursor and the amount of gold uptake and cellular morphology was examined. Identical reactions were carried out with biomass concentration ranging from 25 to 150 g L−1 for a fixed gold(III) ion concentration (1 mM) and the reaction flasks are incubated for 72 h (200 rpm, 37 °C). Samples were analyzed for gold uptake. For the cases with higher gold uptake, transmission electron microscopic analysis was carried out.

Kinetics of gold accumulation was studied using whole resting cells (20 mL, 50 g L−1) for gold (III) chloride (1 mM). At few intervals, the samples were centrifuged to collect the supernatant and the residual gold was measured. Control experiment involves the same concentration of gold precursor added to the buffer and incubated under identical conditions.

The amount of gold atoms present in a single Candida parapsilosis cell was determined by equating the cell count to the amount of gold removal by the cells. Number of yeast cells in the 50 g L−1 cell suspension was determined using haemocytometer. The average number of cells (per mL) was found to be 1.8 (±0.13) × 109 cells. To the reaction flask, varying number of cells was added, to which gold (III) chloride was added to the flasks and kept for incubation at 37 °C, 200 rpm for 72 h. The amount of gold chloride added was 3.51 × 1020 Au atoms. The amount of gold uptake by the cells is determined.

Biosynthesis of gold nanoparticles using the cell free extract

Yeast cultures grown up to 24 h was harvested to remove the growth media using centrifugation (12,800×g, 5 min, 4 °C) and washed twice with MilliQ water, to remove the media components. Phosphate buffer (pH 7, 20 mM) was used to prepare the cell suspension of 50 g L−1 concentration. To the cell suspension prepared with 24 h culture, 1 mM phenyl methyl sulfonyl fluoride was added as a protease inhibitor. Cell suspension was then subjected to ultrasonication (Vibra-cell ultrasonicator) under these conditions (1 s pulse on/off, 35 % amplitude, 4 °C, 10 min). After ultrasonication, the suspension was subjected to centrifugation (12,800×g, 15 min and 4 °C) and the supernatant was collected. The supernatant fraction was the cell free extract used for the biosynthesis of gold nanoparticles.

Cell free extract prepared from resting cells harvested at 24 h was used for the synthesis of gold nanoparticles. To 20 mL of the prepared extract, gold (III) chloride was added to make an overall concentration of 1 mM. The reaction mixture was then kept for incubation at 37 °C, 200 rpm for 72 h.

The concentration of proteins in the cell free extract was estimated using Bradford assay (Bradford 1976). Alcohol dehydrogenase activity (ADH) (Peters et al. 1993) in the extract was assayed using acetophenone as a model substrate. The consumption of NADH during the reaction was monitored spectrophotometrically (V-530 UV/vis Spectrophotometer) at 340 nm and 25 °C using molar extinction coefficient of 6.22 mL μmol−1 cm−1. Similarly, glutathione reductase activity (GR) (Romero-Puertas et al. 2006) in the extract was determined using oxidized glutathione as a substrate and NADPH as a cofactor. One unit (U) of ADH or GR activity is defined as the amount of the enzyme that catalyses the oxidation of 1 μmol of NAD(P)H per minute respectively under the conditions specified.

The cell free extract prepared from the resting cells of Candida parapsilosis ATCC 7330 (fraction I) was used as a reference. The reaction mixture after 72 h was subjected to centrifugation (18,500×g, 60 min, 4 °C). The supernatant fraction containing the unbound proteins (UBP) was collected. The pellet had the gold nanoparticles. The protein concentration in the cell free extracts i.e. fraction I and the unbound protein fraction was estimated using Bradford assay. Both these fractions were further concentrated by lyophilization; these samples of identical protein amounts (50 µg) were denatured and run through sodium dodecyl sulfate–polyacrylamide gel electrophoresis (12 %). The gel was stained initially using Coomassie staining followed by destaining. In order to improve the resolution, the gel was subjected to quick silver staining.

Effect of protein concentration on nanofabrication

Preliminary experiments on biosynthesis of gold nanoparticles were carried out by varying the protein concentration (220–2000 µg mL−1) for the fixed gold (III) chloride (1 mM). Further, identical reactions were carried out with varying protein concentration (220, 330 and 530 µg mL−1), to each of which different concentrations of gold (III) chloride (0.5, 0.75 and 1.0 mM) were added. Experiments were carried out with 20 mL of the prepared cell free extract put in 150 mL conical flask. Reaction flasks were kept for incubation under the standard reaction conditions (37 °C, 200 rpm and 72 h).

Purification of the biosynthesized gold nanoparticles

Gold nanoparticles were purified from the reaction mixture using centrifugation (18,500×g, 60 min, 25 °C), solid nanoparticles were dispersed in MilliQ water and the process was repeated again to obtain gold nanoparticles free from unreacted gold ions.

Effect of pH on the dispersed gold nanoparticles

About 1.5 mL of the gold nanoparticles was subjected to centrifugation (18,500×g, 60 min, 4 °C) and the solid nanoparticles were dispersed in different pH solutions (2, 4, 6, 8, 10, 12). In this study, pH was adjusted in MilliQ water to make different pH solutions (using either hydrochloric acid or sodium hydroxide). Samples were analyzed after the dispersion of gold nanoparticles in respective pH solutions. In addition, long term stability of the better dispersed gold nanoparticles was monitored after 20 months storage at 4 °C.

Catalytic studies

In this model study, pH 12 dispersed gold nanoparticles was used to study the catalytic reduction of 4-nitrophenol (4-NP) using sodium borohydride (NaBH4) as a electron donor at ambient conditions. The progress of the reduction of 4-NP was monitored spectrophotometrically as a decrease in the absorbance of the substrate 4-NP at 400 nm. In the cuvette assay, the final concentrations of the 4-nitrophenol and NaBH4 were made 10−4 and 10−2 M respectively. Typically, this second order reaction was made pseudo first order by keeping NaBH4 concentration 100 fold excess in relative to 4-nitrophenol. About 10 μL (3.3 × 10−9 mol) of the gold nanoparticles was added and the final volume was adjusted to 1 mL using MilliQ water. Identical reactions without the addition of gold nanoparticles were performed as a control experiment. Time course of the catalysis was studied through monitoring the absorbance at 400 nm.

Characterization methods

Characteristic surface plasmon resonance peak of the gold nanoparticles was monitored using JASCO V-530 UV/vis Spectrophotometer. The amount of gold removed by the biomass from the aqueous solution was determined using induced coupled plasma-optical emission spectrometry (Perkin Elmer Optima 5300 DV). The residual concentration of gold in the reaction supernatants was determined by recording the optical emission at λ/nm (267.595), intrinsic to the gold element. Prior to the analysis, instrument was calibrated with known concentration of gold solution. Hydrodynamic diameter, polydispersity index and zeta potential of the gold nanoparticles were determined using Zetasizer 3000 HSA (Malvern Instruments, UK). All these characterization experiments were done in triplicate samples and the results were provided with respective mean value and standard deviation.

Transmission electron microscopy was performed using Philips CM12 Transmission electron microscope to examine the size and morphology of the gold nanoparticles. For better understanding, Image J analysis (Image J 1.46r) was performed to determine the primary particle size from the electron micrographs. The phase identity and crystalline nature of the gold nanoparticles were determined with Bruker Discover D8 diffractometer using Cu (Kα) radiation (λ/Å = 1.5406) at room temperature in the 2θ range from 30° to 100°. The surface chemistry of the lyophilised gold nanoparticles was analysed using FT-IR Eco-ATR Bruker ALPHA spectrometer in the range 600–4000 ν max /cm−1 with a resolution of 4 cm−1. Thermal decomposition of the lyophilized gold nanoparticles was analyzed using thermal gravimetry (NETZSCH STA 449F3) instrument in nitrogen atmosphere at the rate of heating of 5 °C per minute with Al2O3 as a reference sample.

Results

Whole resting cells mediated Au NPs biosynthesis

Effect of culture age

The growth of this yeast in yeast malt broth media (YMB) shows the lag phase (0–6 h), exponential/log phase (6–30 h), stationary phase (30–42 h) and decline phase (42 h and above) (Fig. 1). Fermenting cells which contain AuCl3 did not show any color associated with gold nanoparticles formation. Yeast biomass harvested at different culture ages (24, 36 and 48 h) were incubated with 1 mM AuCl3. UV/vis spectrum analysis of biomass showed the formation of gold nanoparticles as seen spectrophotometrically at ~520–580 nm (surface plasmon resonance, SPR) (Fig. 2a). The initial color of the biomass (pale white) gradually changed and a pinkish coloration was observed with all culture ages (Fig. 2b). Visible inspection of the reaction biomass showed that the pink color is retained with the biomass. The reaction supernatants (free from cell biomass) did not show the spectrophotometric response (~520–580 nm) of gold nanoparticles formation which indicates the lack of extracellular formation of nanoparticles. From quantitative analysis of the reaction supernatants, it was found that the gold removal from the aqueous solution was 77 % with 24 h resting biomass and there was no major difference in the gold removal from the solution with increasing culture ages i.e., 36 h (76 %) and 48 h (77 %).
Fig. 1

Growth curve of Candida parapsilosis ATCC 7330 cultured in a shake flask using Yeast Malt Broth media

Fig. 2

a UV/vis spectrum analysis of the gold nanoparticles biosynthesized using whole cells (24, 36 and 48 h culture cells) of Candida parapsilosis ATCC 7330, b visual representation of the reaction

Transmission electron microscopy analysis of the whole cell mounts shows that the gold nanoparticles were formed using the resting cells (24 h culture) of Candida parapsilosis ATCC 7330 (Fig. 3a) Gold nanoparticles biosynthesized using the resting cells of 24 h culture were spherical in shape. The enlarged micrographs show the uniform distribution of nanoparticles with average size of about 27 nm (Fig. 3b, d) on the whole cells. Energy dispersive analysis of the reaction with resting biomass shows the optical absorption at 2 keV which is a characteristic of the metallic gold which was not observed for the control cells (Fig. 3c; Additional file 1: Figure S1a, b). Experiments showed that the heat killed cells did not produce any discrete nanoparticles (Additional file 1: Figure S2).
Fig. 3

a Transmission electron micrographs of the whole cell mounts after the reaction (Scale bar 1 μm, 3000×), b enlarged micrographs (Scale bar 100 nm, 28,000×), c control cells (Scale bar 1 μm, 5000×) and d frequency based size distribution of gold nanoparticles

Influence of biomass concentration

In the present study, different concentrations of the Candida parapsilosis ATCC 7330 were used for a fixed gold (III) concentration (1 mM). About 79 and 76 % of gold (III) was removed (Additional file 1: Figure S3) from the aqueous solution for the biomass concentrations of 25 and 50 g L−1 respectively and the cell morphology remain almost intact as visualized from electron micrographs (Fig. 4a, b). For the biomass concentrations of 75 and 150 g L−1, the gold uptake decreased to 63 and 52 % respectively.
Fig. 4

Transmission electron microscopic analysis of the gold nanoparticles biosynthesized using a 25 g L−1 and b 50 g L−1 of the biomass concentration against 1 mM AuCl3 (Scale bar 500 nm)

Kinetics of gold accumulation vs. biomineralization of gold nanoparticles

Gold accumulation kinetics was studied for the biomass concentration of 50 g L−1 against 1 mM AuCl3. UV/vis spectrum analysis showed that the biomineralization of gold nanoparticles was increasing with time and more noticeably from 24 to 72 h (Fig. 5a). About 77 % of the gold was bioaccumulated at the end of 72 h (Fig. 5b).
Fig. 5

Kinetics of intracellular formation of gold nanoparticles using resting cells of Candida parapsilosis ATCC 7330 a UV/vis spectrum analysis and b Gold accumulation with respect to time

Optical density (OD) measurements were initially calibrated against the cell number (Additional file 1: Figure S4) such that 1 OD corresponds to 5.4 × 107 cells (0.366 g DCW/L). Assuming that all cells were identical and the cell number was constant during the course of reaction, the maximum number of gold atoms accumulated as nanoparticles within a single cell was found to be in the order of 1010 atoms (Additional file 1: Table S1). Efforts to extract the gold nanoparticles formed within the resting biomass using ultrasonication (Additional file 1: Table S2) gave poor yields of stable Au NPs.

Cell free extract mediated Au NPs biosynthesis

Under identical experimental conditions, the cell free extract of 24 h culture prepared from 50 g L−1 cell suspension was used instead of resting cells. Using UV/vis spectrophotometer, SPR peak (535 nm) corresponding to the formation of gold nanoparticles was observed which was also consistent with the visual inspection (Fig. 6a, b). Gold nanoparticles biosynthesized using the cell free extract were spherical as visualized from microscopic images (Fig. 6c). Using Image J software, the primary particles size from the electron micrographs was found to be 52 nm (considering mainly the larger size fraction) which was well in agreement with the hydrodynamic diameter (Dh) estimation (Dh, 59 nm) and polydispersity index (PDI) of 0.4. Powder X-ray diffraction study depicts the formation of the Au NPs with low surface energy facets such as (111) and (100) (Additional file 1: Figure S5) which represents their face cubic crystalline nature (ICDD card no. 00-04-0784).
Fig. 6

a UV/vis spectrum of the biosynthesis of gold nanoparticles using the cell free extract of Candida parapsilosis ATCC 7300, b Visual inspection and c Electron micrographs of the gold nanoparticles formed using cell free extract (Scale bar 100 nm, 35 K magnification)

Zeta potential of the biosynthesized gold nanoparticles was found to be −24 mV which indicates colloidal stability. Freezed dried pellet of gold nanoparticles showed FT-IR signals at 3271, 2909, 1641, 1537, 1389, 1234 and 1039 cm−1 (Additional file 1: Figure S6). Thermal gravimetric analysis revealed that there was about 10 % weight loss due to the mass change at temperatures in the range of 350–400 °C (Additional file 1: Figure S7). From SDS-PAGE analysis, it was observed that few bands (around 45–60 kDa) diminished in the UBP fraction as compared to fraction 1 (Additional file 1: Figure S8). Protein concentration in fraction 1 was found to be 350 µg mL−1 whereas UBP fraction contains 230 µg mL−1. There was a difference in protein concentration of about 120 µg/mL (34 % of the total proteins) between fraction I and UBP fraction. Relative quantitation of the gel (50 µg of proteins loaded in each well) using densitometry analysis (Image Lab 3.0 software) showed that the intensity of protein bands (labeled as B1, B2 and B3) in unbound proteins fraction were diminished (Additional file 1: Table S3).

Effect of protein concentration on biogenesis of gold nanoparticles

The cell free extract contains a variety of enzymes/proteins and other organic molecules. The protein concentration in the cell free extract prepared from 50 g L−1 cell suspension was 537 µg mL−1. The effect of protein concentration (220–2000 µg mL−1) on the biosynthesis of gold nanoparticles was investigated spectrophotometrically. Characteristic surface plasmon resonance (~520–580 nm) corresponding to the formation of nanogolds (Fig. 7) was seen with lower concentrations of the protein (220, 330 and 530 µg mL−1). Reactions employing higher protein concentration (1500 and 2000 µg mL−1) did not show the SPR bands which indicates that the gold nanoparticles were not formed (Fig. 7). Transmission electron microscopy studies confirmed that the spherical gold nanoparticles formed with 330 and 530 µg mL−1 protein fraction were better dispersed (Fig. 8b, c). However, aggregates of gold nanoparticles were observed with 220 µg mL−1 protein (Fig. 8a) which was also supported by the secondary broad SPR observed in the higher wavelength (Fig. 7).
Fig. 7

UV/vis spectrum of the gold nanoparticles biosynthesized using varying protein concentrations for a fixed gold precursor

Fig. 8

Electron micrographs of the gold nanoparticles biosynthesized through varying protein concentrations (a 0.22; b 0.33 and c 0.53 mg mL−1)for a fixed gold precursor (Scale bar 100 nm)

Furthermore, each of the protein concentrations i.e., 220, 330 and 530 µg mL−1 was titrated against different concentrations of the gold precursor (0.5, 0.75 and 1 mM AuCl3) and the effect on the hydrodynamic diameter, polydispersity index and zeta potential of the gold nanoparticles formed was examined. Spherical Au NPs with particle Dh ranging from 50 to 222 nm were formed (Table 1). Notably, zeta potential of the Au NPs synthesized for all the reactions showed considerable stability i.e., −27 to −20 mV (Table 1).
Table 1

Influence of protein concentration (220–530 µg mL−1) in the cell free extract of Candida parapsilosis ATCC 7330 against different concentrations of gold precursor (0.5–1 mM) towards the biogenesis of gold nanoparticles

Entry

Protein concentration (μg mL−1)

Gold (III) chloride (mM)

Gold nanoparticles

SPR band (nm)

Size

Zeta potential (mV)

Dh (nm)

PDI

1

220 ± 18

0.5

536

57.3 ± 5.8

0.445

−21.4 ± 1.5

2

220 ± 18

0.75

539

109.9 ± 3.

0.308

−27.3 ± 3.2

3

220 ± 18

1.0

543

222 ± 7.7

0.489

−27.8 ± 0.5

4

330 ± 27

0.5

534

56.7 ± 1.1

0.454

−20.8 ± 1.5

5

330 ± 27

0.75

538

71.6 ± 0.6

0.402

−26.2 ± 1.1

6

330 ± 27

1.0

537

50.1 ± 0.6

0.422

−25.5 ± 1.5

7a

530 ± 32

0.5

8

530 ± 32

0.75

546

164.1 ± 3.

0.429

−21.7 ± 1.4

9

530 ± 32

1.0

535

59.2 ± 1.1

0.433

−24 ± 0.3

aNo gold nanoparticles formation

Enzymatic assays showed that the cell free extract was enriched in both the reductase enzymes i.e. alcohol dehydrogenase (ADH, 0.047 U mg−1) and glutathione reductase (GR, 0.024 U mg−1). Experiments showed that at 0.5 mM gold(III) chloride, and a protein concentration of 537 μg mL−1 in the reaction mixture failed to produce Au NPs (entry 7 of Table 1). Assuming the reduction of Au+3 to Au0 is enzyme mediated; the increase in protein concentration should enhance the biosynthesis of Au NPs. On the contrary, increasing protein concentration for a fixed concentration of gold (III) chloride did not improve the biosynthesis of Au NPs. An appropriate control experiment in which heat killed extract was used instead of cell free extract also gave reduced nanogolds (data not shown). Gold nanoparticles produced using cell free extract were polydisperse in nature (Table 1).

Dispersion studies and colloidal stability

Au NPs were purified and the solid nanoparticles were dispersed in MilliQ water. The dispersed Au NPs in water showed increased Dh (76 ± 5 nm) with wavelength maxima of 551 nm as compared to as-prepared nanoparticles (Dh of 59 nm, λmax of 535 nm). The polydispersity index of the water dispersed Au NPs (0.47) did not change much with that of the as-prepared Au NPs with PDI (0.42). Zeta potential of water dispersed Au NPs was about −36 ± 3 mV.

The dispersion behavior of the biosynthesized Au NPs in various pH solutions was monitored using UV/vis spectrophotometer (Fig. 9a). The difference in the SPR absorbance of the dispersed Au NPs was attributed to their dispersion stability which was also consistent with the visual appearances of the samples (Fig. 9b). The colloidal stability of the pH 12 dispersed Au NPs was evidenced by the 10 nm blue shift from λ max of 535 nm (as-prepared) to 525 nm.
Fig. 9

Effect of dispersion of the biosynthesized gold nanoparticles in different pH solutions a surface plasmon resonance analysis b visual inspection of the dispersed samples c dispersion effect on particle hydrodynamic diameter d dispersion effect on zeta potential

Particle size, particle size distribution and zeta potential of the dispersed nanoparticles were measured as a function of pH of the dispersion medium (Fig. 9c, d; Additional file 1: Figure S9). At pH 12, hydrodynamic diameter of the Au NPs was 44.25 with polydispersity index of 0.2 and an increased negative zeta potential of −38.93 mV. Stabilization aspects seems to depend on pH as seen at pH 12 dispersion decreases the polydispersity index of the biosynthesized gold nanoparticles. Electron micrographs confirm the better monodispersity (PDI of 0.2 by dynamic light scattering analysis) of Au NPs in pH 12 solution (Fig. 10b; Additional file 1: Figure S9). Dispersed Au NPs in pH 12 solutions showed a decrease in the diameter and the average size was found to be 32 nm (calculated using Image J software). Storage stability of the pH 12 dispersed gold nanoparticles after 20 months showed a decrease in primary particle size from 32 to 29 nm (Additional file 1: Figure S10) with PDI of 0.2 and zeta potential of −35 mV.
Fig. 10

a A plot showing the linear relationship between ln (At/A0) and time for the dispersed (pH 12) gold nanoparticles mediated catalytic reduction of 4-nitrophenol using sodium borohydride as a reductant and b transmission electron micrographs of the biosynthesized Au NPs dispersed in pH 12 solution (Scale bar 100 nm, 35 k magnification)

For the pH values of 4–10, the Dh is found between 75 and 86 nm and zeta values range from −31 to −42 mV. Dispersion of Au NPs at pH 2 shows gold aggregates with Dh of 8530 nm and zeta potential of 3.5 mV. The dispersal of Au NPs in phosphate buffered saline (pH 7.4) yielded nanoparticles with Dh of 150 ± 42 nm (Additional file 1: Figure S11) and zeta potential of −20.8 ± 1.5 mV. In addition to aqueous solutions, dispersion of biosynthesized Au NPs in organic polar solvents such as dimethylsulfoxide (DMSO) and ethanol was studied. Dispersion in DMSO yielded Au NPs with Dh of 135 ± 6 nm (Additional file 1: Figure S11) and zeta potential of −27 ± 1 mV. In case of ethanol, more gold aggregates were formed with particle Dh of 646 nm (Additional file 1: Figure S11) and zeta potential of −23 mV.

The pH 12 system showed abs520/600 value of 4.40 i.e. more positive stability as compared to the other pH solutions and as-prepared Au NPs (3.25) (Additional file 1: Figure S12). In the present study, the biosynthesized Au NPs dispersed in pH 12 solution was used as a nanocatalyst for the sodium borohydride mediated reduction of 4-nitrophenol which is a well established model reaction (Panigrahi et al. 2007) for evaluating catalytic activity of the metal nanoparticles. The rapid decrease in the absorbance of 4-nitrophenolate ion was observed with the increase in time as compared to the control experiment (Additional file 1: Figures S13, S14) performed in the absence of gold nanoparticles. A linear plot of ln (At/A0) vs. time gave the apparent rate constant (Fig. 10a) (K app ) of 2.3 × 10−3 s−1 (0.138 min−1).

Discussion

Microbial production of nanoparticles involves parameters such as the selection of the suitable biological species and the optimal growth/cultivation conditions necessary for enhanced biosynthesis. When the microbes are challenged with a metallic precursor, mostly aerobic cells use their defense machinery to detoxify the metal which occurs preferably by the reduction of the metal from its native toxic form to the less toxic form (Weast 1984). During this detoxification process, the monomers required for the formation of metal nanoparticles are generated which subsequently undergo nucleation and form nanoparticles. Intracellular accumulation of metals occurs with metabolically active cells (Wang and Chen 2009). More likely, the accumulated gold gets converted to gold nanoparticles within the cell. With resting cells of Candida parapsilosis ATCC 7330, gold nanoparticles formed within the cell and the process could be metabolism dependent. A recent study with the fungus Rhizopus oryzae shows that gold nanoparticles are biosynthesized on the cell wall and the cytoplasmic region (Das et al. 2012b). Reportedly, biogenesis of gold nanoparticles using G. candidum is mediated intracellularly (Mittal et al. 2013). Besides fungal species, intracellular growth of gold nanoparticles are also reported using bacteria (Ivanov et al. 2009) algae (Gangula et al. 2011) and cancerous cell lines (Wang et al. 2013). There is a tremendous interest towards the intracellular synthesis of the metal/alloy nanoparticles using microbes as they are reportedly used as surface enhanced Raman scattering probes (Shamsaie et al. 2007) and heterogeneous catalyst (Deplanche et al. 2012) for chemical reactions.

In this study, the 24 h culture age of Candida parapsilosis ATCC 7330 which corresponds to the late exponential phase was found to be optimum for further studies. Culture age (36 and 48 h) of Candida parapsilosis ATCC 7330 did not show any increase in the gold removal (76 and 77 %) from the aqueous solution as compared to 24 h culture age. Few reports have correlated the richness of enzyme/proteins present in the exponential phase of the microbes to the maximum number of nanoparticles present in situ. An isolated study (Gericke and Pinches 2006a) showed that the number of gold nanoparticles formed per cell decreases with increase in the culture age of V. luteoalbum used. In a separate study, growth phase (exponential phase) of the bacteria is correlated with the maximum amount of gold accumulated within the biomass (Erasmus et al. 2014). With the increase in the biomass concentration, amount of gold (III) loaded into the biomass decreased from 79 % (25 g L−1) to 52 % (150 g L−1). About 5 % decrease in gold uptake is observed with the dried cells of Azolla filiculoides for the increase in biomass concentration from 1 to 9 mg L−1 (Antunes et al. 2001). Interferences between the binding sites for microbial biosorption of metals are one of the possible explanations for the decreased metal uptake. Very likely, an increase in biomass concentration decreases the electrostatic interactions between the metal and the cells (Roussos et al. 2013).

The removal of metals from the aqueous solution is strongly influenced by the contact time between the microbe and the metals (Farhan and Khadom 2015). Quantitative kinetics of the gold accumulation indicated that about 77 % Au+3 was taken up by the cell after 72 h. Visual monitoring shows that the biomineralization of gold nanoparticles increases with time and the same was in consensus with the SPR intensity. An isolated study shows that the bioaccumulation of radioactive gold (H198AuCl4) reaches a maximum limit after 10 h incubation with the yeast Saccharomyces cerevisiae (Panigrahi et al. 2007). Candida parapsilosis ATCC 7330 showed better atom economy (~1010) in terms of the gold atoms bioaccumulated within a single yeast cell as compared to AP22 and CCFY-100 strains of the yeast Saccharomyces cerevisiae where 107 radioactive gold atoms (198Au) are accumulated in the form of nanoparticles of size (15–20 nm) within each cell (Sen et al. 2011).

Apart from resting cells, microbial resources such as crude extracts, cell free filtrates, and purified enzymes/proteins are also used to synthesize metal nanoparticles. Using cell free extracts of Candida parapsilosis ATCC 7330, spherical gold nanoparticles with hydrodynamic diameter of 50–220 nm was obtained by varying the reaction stoichiometry between the gold precursor (0.5–1 mM) and the protein concentration (220–530 µg/mL). The biosynthesis of spherical and non-spherical shaped gold nanoparticles in the size of 20–80 nm using the cytosolic extract of Candida albicans (Chauhan et al. 2011) is reported. The possible surface chemistry involved in stabilization of gold nanoparticles (lyophilized sample) was studied using FT-IR analysis. A broad band at 3271 cm−1 indicated the N–H stretching of the primary amines in the protein molecules (Correa-Llantén et al. 2013). The FT-IR bands noticed at 1641, 1537, 1234 cm−1 corresponded to the amide I, amide II and amide III bands of peptide units of polypeptide/proteins respectively (Rajeshkumar et al. 2013; Aryal et al. 2006; Shankar et al. 2003). A band at 1389 cm−1 corresponded to the symmetric stretching of the carboxylate (COO) groups (Aryal et al. 2006). A notable band was seen at 1039 cm−1 which indicated the C-N stretching vibrations possibly from aliphatic amines of the proteins (Rajeshkumar et al. 2013). This analysis indicated that the peptide/protein molecules could be involved in capping the Au NPs formed. Green synthesis of nanoparticles using microbial extracts are reported to synthesize stable gold nanoparticles where peptide/protein molecules are capping the nanoparticles (Kitching et al. 2014). Thermal decomposition studies of the freeze dried Au NPs samples suggested the presence of capping agents which decomposes around 350–400 °C. A similar finding is reported in a biogenic approach using C. albicans (Ahmad et al. 2013), where the protein biomolecules are shown to stabilize the nanoparticles produced. In addition, SDS-PAGE analysis suggest that cellular proteins are involved in the stabilization of the gold nanoparticles biosynthesized using the cell free extract of Candida parapsilosis ATCC 7330.

The two main events in gold nanoparticles formation in the yeast, viz. reduction and stabilization (Capping) are recognized but their mechanism is not completely understood (Duran et al. 2011; Faramarzi and Sadighi 2013; Hulkoti and Taranath 2014; Singh et al. 2015). The cell free extract used for the biosynthesis of gold nanoparticles was enriched in alcohol dehydrogenase (ADH) and glutathione reductase (GR) enzymes. It is known that ADH (Drauz et al. 2012) mediates the enzymatic reduction of carbonyl compounds using NAD(P)H whereas GR (Penninckx 2002) catalyzes the formation of reduced glutathione from oxidized glutathione using NADPH. Enzymes such as nitrate reductase (Kalimuthu et al. 2008), hydrogenase (Riddin et al. 2009), sulfate reductase (Ahmad et al. 2002), phenol oxidizing enzymes namely laccase, tyrosinase, Mn-peroxidase (Vetchinkina et al. 2014), alpha-amylase (Manivasagan et al. 2015) and few others are implicated in the bioreduction of Au(III) to Au(0). Vaidyanathan et al. (2010) have shown that optimizing the activity of nitrate reductase enhanced the silver nanoparticles production using B. licheniformis. Scott et al. (2008) proposed that the metallic gold nanoparticles formation occurs at the active site of NADPH dependent glutathione reductase. E. coli cells bioengineered with bacterial glycerol dehydrogenase are reported for in situ biocatalytic synthesis of gold nanoparticles using NADH as a cofactor (Niide et al. 2011). Reduction of gold precursor was observed even with heat denatured cell free extract which indicate that the process is not entirely due to enzymatic reactions. Thus, multiple reduction/stabilization reactions do occur and produce the reduced nanogolds. This was further supported by the experiment where increasing protein concentration for a fixed metal precursor did not enhance the formation of gold nanoparticles and the same is consistent with earlier reports (Das et al. 2012a; Tan et al. 2010). Thus, direct correlation to reductase activity may not be precise but the total protein concentration likely influences the formation of stable Au NPs with moderate polydispersity.

It is also established that the fungal/yeast species generates metal nanoparticles with broad size distribution (Kitching et al. 2014). The presence of more than one nucleation event during biogenic nanofabrication contributes to polydispersity. The utility of the polydisperse gold nanoparticles is limited due to the overlapping properties of the varying sizes of the nanoparticles produced. Achieving dispersions of gold nanoparticles with narrow size distribution is important. Dispersion of the biosynthesized gold nanoparticles in pH 12 solution improved the monodispersity of the gold nanoparticles. Long term storage of pH 12 dispersed gold nanoparticles for about 20 months at 4 °C show improved dissolution of nanoparticles due to a decrease in the size of the dispersed nanoparticles from 32 to 29 nm (as calculated from electron micrographs) although there was no significant change in the polydispersity index and zeta potential of the nanoparticles. In basic conditions, the deprotonation of the Au-OH groups on the surface of the nanoparticles (Pfeiffer et al. 2014) provides electrostatic repulsive forces improving the dispersion of gold nanoparticles. In the chemical approach, adjusting the reaction to alkaline pH is reported to produce monodisperse gold nanoparticles with controlled particle size distribution (Ji et al. 2007; Kumar et al. 2007; Yang et al. 2007). On the other hand, less positive zeta values (3.5 ± 0.5 mV) of the pH 2 dispersed gold nanoparticles indicate that the thickness of the electrical double layer is drastically reduced (Sennett and Olivier 1965) and therefore as a result, strong aggregation of gold nanoparticles was seen which may be due to the increased Van der Waal’s attractive forces as compared to the stabilizing forces (Nel et al. 2009). Similar observation is reported in the aggregation behavior of biologically synthesized silver nanoparticles (Prathna et al. 2011). For the dispersion of Au NPs in polar solvents such as DMSO and ethanol, the varying agglomeration behavior was observed which could be attributed to the difference in the dielectric constants among the solvents. The results are in accordance with a recent report (Burrows et al. 2014), which states that the decrease in the dielectric constant (DMSO, 48 and ethanol, 24) is expected to decrease the repulsive forces between the nanoparticles and thus results in more aggregation. Colloidal stability of Au NPs is evaluated on the basis of the stability parameter (Ivanov et al. 2009) derived from surface plasmon resonance assay i.e., the ratio of the absorbance measured at 520 nm to that of 600 nm. Surface Plasmon resonance assay confirmed the better dispersion stability of biosynthesized gold nanoparticles in pH 12 solution as compared to other pH solutions. In the presence of sodium borohydride, dispersed gold nanoparticles (in pH 12 solution) was catalytically active as the substrate 4-nitrophenol was found decreasing with time in the spectrophotometric assay and the calculated rate constant was similar to the reported (Zayed and Eisa 2014) values (3.1 × 10−3 s−1) for Au NPs of 32 nm.

In summary, a one-pot sustainable method employing the use of yeast cells, Candida parapsilosis ATCC 7330 as a mild reagent for the biosynthesis of gold nanoparticles was established. Cell free extracts gave better gold nanoparticles of size (50–220 nm) whereas resting cells yielded gold nanoparticles accumulated within the cell. The formation of nanoparticles using the cell free extract depends on total cellular protein concentration and not only enzymatic activity of redox enzymes. This is the first detailed report to address the dispersion behavior of biosynthesized gold nanoparticles in different matrices. Dispersion of the biosynthesized gold nanoparticles in pH 12 solution (32 nm Au NPs) improves the particle monodispersity which is demonstrated via the size dependent catalytic activity for the reduction of 4-nitrophenol.

Abbreviations

YMB: 

yeast malt broth

AuCl3

gold (III) chloride

4-NP: 

4-nitrophenol

NaBH4

sodium borohydride

OD: 

optical density

Au NPs: 

gold nanoparticles

SPR: 

surface plasmon resonance

Dh

hydrodynamic diameter

PDI: 

polydispersity index

ADH: 

alcohol dehydrogenase

GR: 

glutathione reductase

DMSO: 

dimethyl sulfoxide

NADH: 

reduced form of nicotinamide adenine dinucleotide

NAD(P)H: 

reduced form of nicotinamide adenine dinucleotide phosphate

Declarations

Authors’ contributions

All the authors conceived the research work. SK carried out the experiments and wrote the manuscript. All authors read and approved the final manuscript.

Acknowledgements

SK extends his thanks to Indian Institute of Technology Madras for HTRA-fellowship. SN thanks the Department of Science and Technology, Government of India for the FAST TRACK fellowship. The authors acknowledge the Central XRD, Central TEM facility of IITM and Chem lab of Central Leather Research Institute for particle size measurements.

Competing interests

The authors declare that they have no competing interests.

Ethics approval

This article does not contain any studies with human participants or animals performed by any of the authors.

Funding information

This research was funded by Board of Research in Nuclear Sciences (BRNS), Government of India.

Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), 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.

Authors’ Affiliations

(1)
Laboratory of Bioorganic Chemistry, Department of Biotechnology, Indian Institute of Technology Madras
(2)
Faculty of Allied Health Sciences, Chettinad Academy of Research and Education
(3)
National Center for Catalysis Research, Indian Institute of Technology Madras
(4)
Centre for NEMS and Nanophotonics, Indian Institute of Technology Madras

References

  1. Agnihotri M, Joshi S, Kumar AR, Zinjarde S, Kulkarni S (2009) Biosynthesis of gold nanoparticles by the tropical marine yeast Yarrowia lipolytica NCIM 3589. Mater Lett 63(15):1231–1234. doi:10.1016/j.matlet.2009.02.042 View ArticleGoogle Scholar
  2. Ahmad A, Mukherjee P, Mandal D, Senapati S, Khan MI, Kumar R, Sastry M (2002) Enzyme mediated extracellular synthesis of CdS nanoparticles by the fungus, Fusarium oxysporum. J Am Chem Soc 124(41):12108–12109. doi:10.1021/ja027296o PubMedView ArticleGoogle Scholar
  3. Ahmad T, Wani IA, Manzoor N, Ahmed J, Asiri AM (2013) Biosynthesis, structural characterization and antimicrobial activity of gold and silver nanoparticles. Colloids Surf B 107:227–234. doi:10.1016/j.colsurfb.2013.02.004 View ArticleGoogle Scholar
  4. Antunes APM, Watkins GM, Duncan JR (2001) Batch studies on the removal of gold(III) from aqueous solution by Azolla filiculoides. Biotechnol Lett 23(4):249–251. doi:10.1023/A:1005633608727 View ArticleGoogle Scholar
  5. Aryal S, Remant BK, Dharmaraj N, Bhattarai N, Kim CH, Kim HY (2006) Spectroscopic identification of S-Au interaction in cysteine capped gold nanoparticles. Spectrochim Acta Mol Biomol Spectrosc 63(1):160–163. doi:10.1016/j.saa.2005.04.048 View ArticleGoogle Scholar
  6. Boroumand Moghaddam A, Namvar F, Moniri M, Md Tahir P, Azizi S, Mohamad R (2015) Nanoparticles biosynthesized by fungi and yeast: a review of their preparation, properties, and medical applications. Molecules 20(9):16540–16565. doi:10.3390/molecules200916540 PubMedView ArticleGoogle Scholar
  7. Bradford MM (1976) A rapid and sensitive method for the quantitation of microgram quantities of protein utilizing the principle of protein-dye binding. Anal Biochem 72(1):248–254. doi:10.1016/0003-2697(76)90527-3 PubMedView ArticleGoogle Scholar
  8. Burrows ND, Kesselman E, Sabyrov K, Stemig A, Talmon Y, Penn RL (2014) Crystalline nanoparticle aggregation in non-aqueous solvents. CrystEngComm 16(8):1472–1481. doi:10.1039/C3CE41584H View ArticleGoogle Scholar
  9. Chauhan A, Zubair S, Tufail S, Sherwani A, Sajid M, Raman SC, Azam A, Owais M (2011) Fungus-mediated biological synthesis of gold nanoparticles: potential in detection of liver cancer. Int J Nanomed 6:2305–2319. doi:10.2147/IJN.S23195 Google Scholar
  10. Correa-Llantén DN, Muñoz-Ibacache SA, Castro ME, Muñoz PA, Blamey JM (2013) Gold nanoparticles synthesized by Geobacillus sp. strain ID17 a thermophilic bacterium isolated from Deception Island, Antarctica. Microb Cell Fact 12:75. doi:10.1186/1475-2859-12-75 PubMedPubMed CentralView ArticleGoogle Scholar
  11. Dameron CT, Smith BR, Winge DR (1989) Glutathione-coated cadmium-sulfide crystallites in Candida glabrata. J Biol Chem 264(29):17355–17360PubMedGoogle Scholar
  12. Das SK, Dickinson C, Lafir F, Brougham DF, Marsili E (2012a) Synthesis, characterization and catalytic activity of gold nanoparticles biosynthesized with Rhizopus oryzae protein extract. Green Chem 14(5):1322–1334. doi:10.1039/C2GC16676C View ArticleGoogle Scholar
  13. Das SK, Liang J, Schmidt M, Laffir F, Marsili E (2012b) Biomineralization mechanism of gold by zygomycete fungi Rhizopus oryzae. ACS Nano 6(7):6165–6173. doi:10.1021/nn301502s PubMedView ArticleGoogle Scholar
  14. Deplanche K, Merroun ML, Casadesus M, Tran DT, Mikheenko IP, Bennett JA, Zhu J, Jones IP, Attard GA, Wood J, Selenska-Pobell S, Macaskie LE (2012) Microbial synthesis of core/shell gold/palladium nanoparticles for applications in green chemistry. J R Soc Interface 9(72):1705–1712. doi:10.1098/rsif.2012.0003 PubMedPubMed CentralView ArticleGoogle Scholar
  15. Dighton J, White J (2005) The fungal community: its organization and role in the Ecosystem, 3rd edn. CRC Press, Boca ratonView ArticleGoogle Scholar
  16. Dixit R, Wasiullah Malaviya D, Pandiyan K, Singh U, Sahu A, Shukla R, Singh B, Rai J, Sharma P, Lade H, Paul D (2015) Bioremediation of heavy metals from soil and aquatic environment: an overview of principles and criteria of fundamental processes. Sustainability 7(2):2189. doi:10.3390/su7022189 View ArticleGoogle Scholar
  17. Drauz K, Gröger H, May O (2012) Enzyme catalysis in organic synthesis: a comprehensive handbook. Wiley-VCH, HobokenView ArticleGoogle Scholar
  18. Duran N, Marcato PD, Duran M, Yadav A, Gade A, Rai M (2011) Mechanistic aspects in the biogenic synthesis of extracellular metal nanoparticles by peptides, bacteria, fungi, and plants. Appl Microbiol Biotechnol 90(5):1609–1624. doi:10.1007/s00253-011-3249-8 PubMedView ArticleGoogle Scholar
  19. Erasmus M, Cason ED, Marwijk J, Botes E, Gericke M, Heerden E (2014) Gold nanoparticle synthesis using the thermophilic bacterium Thermus scotoductus SA-01 and the purification and characterization of its unusual gold reducing protein. Gold Bull 47(4):245–253. doi:10.1007/s13404-014-0147-8 View ArticleGoogle Scholar
  20. Eustis S, El-Sayed MA (2006) Why gold nanoparticles are more precious than pretty gold: noble metal surface plasmon resonance and its enhancement of the radiative and nonradiative properties of nanocrystals of different shapes. Chem Soc Rev 35(3):209–217. doi:10.1039/B514191E PubMedView ArticleGoogle Scholar
  21. Faramarzi MA, Sadighi A (2013) Insights into biogenic and chemical production of inorganic nanomaterials and nanostructures. Adv Colloid Interface Sci 189–190:1–20. doi:10.1016/j.cis.2012.12.001 PubMedView ArticleGoogle Scholar
  22. Farhan SN, Khadom AA (2015) Biosorption of heavy metals from aqueous solutions by Saccharomyces cerevisiae. Int J Ind Chem 6(2):119–130. doi:10.1007/s40090-015-0038-8 View ArticleGoogle Scholar
  23. Gadd GM (2010) Metals, minerals and microbes: geomicrobiology and bioremediation. Microbiology (Reading, England) 156(Pt 3):609–643. doi:10.1099/mic.0.037143-0 View ArticleGoogle Scholar
  24. Gangula A, Podila R, Karanam L, Janardhana C, Rao AM (2011) Catalytic reduction of 4-nitrophenol using biogenic gold and silver nanoparticles derived from Breynia rhamnoides. Langmuir 27(24):15268–15274. doi:10.1021/la2034559 PubMedView ArticleGoogle Scholar
  25. Gericke M, Pinches A (2006a) Biological synthesis of metal nanoparticles. Hydrometallurgy 83(1–4):132–140. doi:10.1016/j.hydromet.2006.03.019 View ArticleGoogle Scholar
  26. Gericke M, Pinches A (2006b) Microbial production of gold nanoparticles. Gold Bull 39(1):22–28. doi:10.1007/bf03215529 View ArticleGoogle Scholar
  27. Hulkoti NI, Taranath TC (2014) Biosynthesis of nanoparticles using microbes—a review. Colloids Surf B 121:474–483. doi:10.1016/j.colsurfb.2014.05.027 View ArticleGoogle Scholar
  28. Ivanov MR, Bednar HR, Haes AJ (2009) Investigations of the mechanism of gold nanoparticle stability and surface functionalization in capillary electrophoresis. ACS Nano 3(2):386–394. doi:10.1021/nn8005619 PubMedPubMed CentralView ArticleGoogle Scholar
  29. Jha AK, Prasad K, Kulkarni AR (2009a) Synthesis of TiO2 nanoparticles using microorganisms. Colloids Surf B 71(2):226–229. doi:10.1016/j.colsurfb.2009.02.007 View ArticleGoogle Scholar
  30. Jha AK, Prasad K, Prasad K (2009b) A green low-cost biosynthesis of Sb2O3 nanoparticles. Biochem Eng J 43(3):303–306. doi:10.1016/j.bej.2008.10.016 View ArticleGoogle Scholar
  31. Ji X, Song X, Li J, Bai Y, Yang W, Peng X (2007) Size control of gold nanocrystals in citrate reduction: the third role of citrate. J Am Chem Soc 129(45):13939–13948. doi:10.1021/ja074447k PubMedView ArticleGoogle Scholar
  32. Kaliaperumal T (2011) PhD Thesis, Indian Institute of Technology MadrasGoogle Scholar
  33. Kaliaperumal T, Kumar S, Gummadi SN, Chadha A (2010) Asymmetric synthesis of (S)-ethyl-4-chloro-3-hydroxybutanoate using Candida parapsilosis ATCC 7330. J Ind Microbiol Biotechnol 37(2):159–165PubMedView ArticleGoogle Scholar
  34. Kalimuthu K, Suresh Babu R, Venkataraman D, Bilal M, Gurunathan S (2008) Biosynthesis of silver nanocrystals by Bacillus licheniformis. Colloids Surf B 65(1):150–153. doi:10.1016/j.colsurfb.2008.02.018 View ArticleGoogle Scholar
  35. Kitching M, Ramani M, Marsili E (2014) Fungal biosynthesis of gold nanoparticles: mechanism and scale up. Microb Biotechnol. doi:10.1111/1751-7915.12151 PubMedPubMed CentralGoogle Scholar
  36. Kumar S, Gandhi KS, Kumar R (2007) Modeling of formation of gold nanoparticles by citrate method. Ind Eng Chem Res 46(10):3128–3136. doi:10.1021/ie060672j View ArticleGoogle Scholar
  37. Mahajabeen P, Chadha A (2013) A novel green route for the synthesis of N-phenylacetamides, benzimidazoles and acridinediones using Candida parapsilosis ATCC 7330. RSC Adv 3(44):21972–21980. doi:10.1039/C3RA44058C View ArticleGoogle Scholar
  38. Manivasagan P, Venkatesan J, Kang KH, Sivakumar K, Park SJ, Kim SK (2015) Production of α-amylase for the biosynthesis of gold nanoparticles using Streptomyces sp. MBRC-82. Int J Biol Macromol 72:71–78. doi:10.1016/j.ijbiomac.2014.07.045 PubMedView ArticleGoogle Scholar
  39. Mittal AK, Kaler A, Mulay AV, Banerjee UC (2013) Synthesis of gold nanoparticles using whole cells of Geotrichum candidum. J Nanoparticles 2013:6. doi:10.1155/2013/150414 View ArticleGoogle Scholar
  40. Mukherjee P, Ahmad A, Mandal D, Senapati S, Sainkar SR, Khan MI, Ramani R, Parischa R, Ajayakumar PV, Alam M, Sastry M, Kumar R (2001) Bioreduction of AuCl4 ions by the fungus, Verticillium sp. and surface trapping of the gold nanoparticles formed. Angew Chem Int 40(19):3585–3588. doi:10.1002/1521-3773(20011001)40:19<3585:AID-ANIE3585>3.0.CO;2-K View ArticleGoogle Scholar
  41. Nel AE, Madler L, Velegol D, Xia T, Hoek EMV, Somasundaran P, Klaessig F, Castranova V, Thompson M (2009) Understanding biophysicochemical interactions at the nano-bio interface. Nat Mater 8(7):543–557. doi:10.1038/nmat2442 PubMedView ArticleGoogle Scholar
  42. Niide T, Goto M, Kamiya N (2011) Biocatalytic synthesis of gold nanoparticles with cofactor regeneration in recombinant Escherichia coli cells. Chem Commun 47(26):7350–7352View ArticleGoogle Scholar
  43. Panigrahi S, Basu S, Praharaj S, Pande S, Jana S, Pal A, Ghosh SK, Pal T (2007) Synthesis and size-selective catalysis by supported gold nanoparticles: study on heterogeneous and homogeneous catalytic process. J Phys Chem C 111(12):4596–4605. doi:10.1021/jp067554u View ArticleGoogle Scholar
  44. Penninckx MJ (2002) An overview on glutathione in Saccharomyces versus non-conventional yeasts. FEMS Yeast Res 2(3):295–305. doi:10.1016/s1567-1356(02)00081-8 PubMedGoogle Scholar
  45. Peters J, Zelinski T, Minuth T, Kula MR (1993) Synthetic applications of the carbonyl reductases isolated from Candida parapsilosis and Rhodococcus erythropolis. Tetrahedron Asymmetry 4(7):1683–1692View ArticleGoogle Scholar
  46. Pfeiffer C, Rehbock C, Hühn D, Carrillo-Carrion C, de Aberasturi DJ, Merk V, Barcikowski S, Parak WJ (2014) Interaction of colloidal nanoparticles with their local environment: the (ionic) nanoenvironment around nanoparticles is different from bulk and determines the physico-chemical properties of the nanoparticles. J R Soc Interface 11(96):20130931. doi:10.1098/rsif.2013.0931 PubMedPubMed CentralView ArticleGoogle Scholar
  47. Philip D (2009) Biosynthesis of Au, Ag and Au-Ag nanoparticles using edible mushroom extract. Spectrochim Acta Mol Biomol Spectrosc 73(2):374–381. doi:10.1016/j.saa.2009.02.037 View ArticleGoogle Scholar
  48. Prathna TC, Chandrasekaran N, Mukherjee A (2011) Studies on aggregation behaviour of silver nanoparticles in aqueous matrices: effect of surface functionalization and matrix composition. Colloids Surf A 390(1–3):216–224. doi:10.1016/j.colsurfa.2011.09.047 View ArticleGoogle Scholar
  49. Rajeshkumar S, Malarkodi C, Gnanajobitha G, Paulkumar K, Vanaja M, Kannan C, Annadurai G (2013) Seaweed-mediated synthesis of gold nanoparticles using Turbinaria conoides and its characterization. J Nanostructure Chem 3(1):1–7. doi:10.1186/2193-8865-3-44 View ArticleGoogle Scholar
  50. Reith F, Lengke MF, Falconer D, Craw D, Southam G (2007) The geomicrobiology of gold. ISME J 1(7):567–584. doi:10.1038/ismej.2007.75 PubMedView ArticleGoogle Scholar
  51. Riddin TL, Govender Y, Gericke M, Whiteley CG (2009) Two different hydrogenase enzymes from sulphate-reducing bacteria are responsible for the bioreductive mechanism of platinum into nanoparticles. Enzyme Microb Technol 45(4):267–273. doi:10.1016/j.enzmictec.2009.06.006 View ArticleGoogle Scholar
  52. Romero-Puertas MC, Corpas FJ, Sandalio LM, Leterrier M, Rodríguez-Serrano M, Del Río LA, Palma JM (2006) Glutathione reductase from pea leaves: response to abiotic stress and characterization of the peroxisomal isozyme. New Phytol 170(1):43–52PubMedView ArticleGoogle Scholar
  53. Roussos S, Soccol CR, Pandey A, Augur C (2013) New horizons in biotechnology. Springer, NetherlandsGoogle Scholar
  54. Scott D, Toney M, Muzikar M (2008) Harnessing the mechanism of glutathione reductase for synthesis of active site bound metallic nanoparticles and electrical connection to electrodes. J Am Chem Soc 130(3):865–874. doi:10.1021/ja074660g PubMedView ArticleGoogle Scholar
  55. Sen K, Sinha P, Lahiri S (2011) Time dependent formation of gold nanoparticles in yeast cells: a comparative study. Biochem Eng J 55(1):1–6. doi:10.1016/j.bej.2011.02.014 View ArticleGoogle Scholar
  56. Sennett P, Olivier JP (1965) Colloidal dispersions, electrokinetic effects, and the concept of zeta potential. Ind Eng Chem 57(8):32–50. doi:10.1021/ie50668a007 View ArticleGoogle Scholar
  57. Seshadri S, Saranya K, Kowshik M (2011) Green synthesis of lead sulfide nanoparticles by the lead resistant marine yeast, Rhodosporidium diobovatum. Biotechnol Prog 27(5):1464–1469. doi:10.1002/btpr.651 PubMedView ArticleGoogle Scholar
  58. Shamsaie A, Jonczyk M, Sturgis J, Paul Robinson J, Irudayaraj J (2007) Intracellularly grown gold nanoparticles as potential surface-enhanced Raman scattering probes. J Biomed Opt 12(2):020502. doi:10.1117/1.2717549 PubMedView ArticleGoogle Scholar
  59. Shankar SS, Ahmad A, Pasricha R, Sastry M (2003) Bioreduction of chloroaurate ions by geranium leaves and its endophytic fungus yields gold nanoparticles of different shapes. J Mater Chem 13(7):1822–1826. doi:10.1039/B303808B View ArticleGoogle Scholar
  60. Sharma SK, Mudhoo A (2010) Green chemistry for environmental sustainability. CRC Press, Boca RatonGoogle Scholar
  61. Singh OV (2015) Bio-nanoparticles: biosynthesis and sustainable biotechnological implications. Wiley, HobokenView ArticleGoogle Scholar
  62. Singh R, Shedbalkar U, Wadhwani S, Chopade B (2015) Bacteriagenic silver nanoparticles: synthesis, mechanism, and applications. App Microbiol Biotechnol 99(11):4579–4593. doi:10.1007/s00253-015-6622-1 View ArticleGoogle Scholar
  63. Tan YN, Lee JY, Wang DIC (2010) Uncovering the design rules for peptide synthesis of metal nanoparticles. J Am Chem Soc 132(16):5677–5686PubMedView ArticleGoogle Scholar
  64. Vaidyanathan R, Gopalram S, Kalishwaralal K, Deepak V, Pandian SR, Gurunathan S (2010) Enhanced silver nanoparticle synthesis by optimization of nitrate reductase activity. Colloids Surf B 75(1):335–341. doi:10.1016/j.colsurfb.2009.09.006 View ArticleGoogle Scholar
  65. Venkataraman S, Chadha A (2015) Biocatalytic deracemisation of aliphatic beta-hydroxy esters: improving the enantioselectivity by optimisation of reaction parameters. J Ind Microbiol Biotechnol 42(2):173–180. doi:10.1007/s10295-014-1558-5 PubMedView ArticleGoogle Scholar
  66. Vetchinkina EP, Loshchinina EA, Burov AM, Dykman LA, Nikitina VE (2014) Enzymatic formation of gold nanoparticles by submerged culture of the basidiomycete Lentinus edodes. J Biotechnol 182–183:37–45. doi:10.1016/j.jbiotec.2014.04.018 PubMedView ArticleGoogle Scholar
  67. Virkutyte J, Varma RS (2013) Green synthesis of nanomaterials: environmental aspects sustainable nanotechnology and the environment: advances and achievements. In: ACS symposium series, vol 1124. American Chemical Society, p 11–39Google Scholar
  68. Wang J, Chen C (2009) Biosorbents for heavy metals removal and their future. Biotechnol Adv 27(2):195–226. doi:10.1016/j.biotechadv.2008.11.002 PubMedView ArticleGoogle Scholar
  69. Wang J, Zhang G, Li Q, Jiang H, Liu C, Amatore C, Wang X (2013) In vivo self-bio-imaging of tumors through in situ biosynthesized fluorescent gold nanoclusters. Sci Rep 3:1157. doi:10.1038/srep01157 PubMedPubMed CentralGoogle Scholar
  70. Weast RC (1984) CRC handbook of chemistry and physics, 64th edn. CRC Press, Boca RatonGoogle Scholar
  71. Yadav A, Kon K, Kratosova G, Duran N, Ingle AP, Rai M (2015) Fungi as an efficient mycosystem for the synthesis of metal nanoparticles: progress and key aspects of research. Biotechnol Lett 37(11):2099–2120. doi:10.1007/s10529-015-1901-6 PubMedView ArticleGoogle Scholar
  72. Yang S, Wang Y, Wang Q, Zhang R, Ding B (2007) UV irradiation induced formation of Au nanoparticles at room temperature: the case of pH values. Colloids Surf A 301(1–3):174–183. doi:10.1016/j.colsurfa.2006.12.051 Google Scholar
  73. Zayed MF, Eisa WH (2014) Phoenix dactylifera L. leaf extract phytosynthesized gold nanoparticles; controlled synthesis and catalytic activity. Spectrochim Acta Mol Biomol Spectrosc 121:238–244. doi:10.1016/j.saa.2013.10.092 View ArticleGoogle Scholar

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