Investigation of the Interaction between Patulin and Human Serum Albumin by a Spectroscopic Method, Atomic Force Microscopy, and Molecular Modeling

Yuqin, Li; Guirong, You; Zhen, Yang; Caihong, Liu; Baoxiu, Jia; Jiao, Chen; Yurong, Guo

doi:https://doi.org/10.1155/2014/734850

BioMed Research International

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Abstract Introduction Materials and Methods Results and Discussion Conclusions Abbreviations References Copyright Related Articles

Research Article | Open Access

Volume 2014 | Article ID 734850 | https://doi.org/10.1155/2014/734850

Investigation of the Interaction between Patulin and Human Serum Albumin by a Spectroscopic Method, Atomic Force Microscopy, and Molecular Modeling

Li Yuqin,¹You Guirong,¹Yang Zhen,²Liu Caihong,¹Jia Baoxiu,¹Chen Jiao,³and Guo Yurong⁴

Academic Editor: Kazuma Ogawa

Received27 Feb 2014

Accepted08 Apr 2014

Published08 Jul 2014

Abstract

The interaction of patulin with human serum albumin (HSA) was studied in vitro under normal physiological conditions. The study was performed using fluorescence, ultraviolet-visible spectroscopy (UV-Vis), circular dichroism (CD), atomic force microscopy (AFM), and molecular modeling techniques. The quenching mechanism was investigated using the association constants, the number of binding sites, and basic thermodynamic parameters. A dynamic quenching mechanism occurred between HSA and patulin, and the binding constants (K) were 2.60 × 10⁴, 4.59 × 10⁴, and 7.01 × 10⁴ M⁻¹ at 288, 300, and 310 K, respectively. Based on fluorescence resonance energy transfer, the distance between the HSA and patulin was determined to be 2.847 nm. The , , and values across various temperatures indicated that hydrophobic interaction was the predominant binding force. The UV-Vis and CD results confirmed that the secondary structure of HSA was altered in the presence of patulin. The AFM results revealed that the individual HSA molecule dimensions were larger after interaction with patulin. In addition, molecular modeling showed that the patulin-HSA complex was stabilized by hydrophobic and hydrogen bond forces. The study results suggested that a weak intermolecular interaction occurred between patulin and HSA. Overall, the results are potentially useful for elucidating the toxigenicity of patulin when it is combined with the biomolecular function effect, transmembrane transport, toxicological, testing and other experiments.

1. Introduction

Patulin is a toxic secondary metabolite produced by a variety of food spoilage fungi, particularly by Penicillium, Aspergillus genera, and Byssochlamys species [1]. Different foods, including fruits and grains, especially apple and its juice, can be affected by these fungi and become contaminated with patulin [2]. The highest patulin production has been observed at storage temperatures between 4 and 25°C [3–5]. Patulin has a strong affinity for sulfhydryl groups, inhibiting the activity of many enzymes [6, 7]. It also has strong antibiotic properties [8] and was used to treat the common cold in the 1940s. Acute toxicity after high dosing in animals is expressed as agitation, convulsions, dyspnea, pulmonary congestion, edema, ulceration, hyperemia, and gastrointestinal tract distension [9–11]. Nausea, vomiting, gastrointestinal disturbance, and kidney damage have been reported in humans [12, 13]. Patulin has been reported to be a genotoxic, reprotoxic, embryotoxic, and immunosuppressive compound [14–18]. To establish guidelines for human exposure to patulin, the JECFA lowered the provisional maximum tolerable daily intake (PMTDI) of patulin from 1 to 0.4 mg/kg body mass/day based on a no-observed-effect level (NOEL) of 43 mg/kg body mass/day and the use of a 100-fold safety factor [6].

Human serum albumin (HSA) containing 585 amino acid residues is the most abundant protein constituent of the circulatory system, contributing significantly to physiological functions as carrier proteins [19]. HSA contains three homologous α-helical domains (I-III). Each of these domains is divided into A and B subdomains that contain six and four α-helices, respectively [20, 21]. Based solely on this sole structure, HSA has an ability to bind an unusually broad spectrum of ligands such as inorganic ions, various drugs, amino acids, and fatty acids [22]. Binding to HSA facilitates the transport of these ligands throughout the circulation [23]. Moreover, these bindings appear to affect the secondary and tertiary structure of albumin [24]. Without a doubt, the interaction of any toxicant with HSA affects the transport of nutrients and drugs. Recently, studies have been conducted on the binding of organic contaminants or toxins to HSA, for example, Arazine, ochratoxin A, methyl parathion, arsenic, perfluorooctanoic acid and phthalate esters, deoxynivalenol, and 2-mercaptobenzimidazole [25–32].

In this study, the interaction of patulin with HSA was investigated using steady-state and time-resolved fluorescence spectroscopy, UV-Vis spectroscopy, circular dichroism (CD) spectroscopy, atomic force microscopy (AFM), and molecular modeling.

2. Materials and Methods

2.1. Materials

HSA (fatty acid free < 0.05%) was purchased from Sigma Chemical Company (USA), and patulin (Figure 1, analytical grade) was purchased from J & K Technology Co., Ltd (USA). A 0.05 mol·L⁻¹ Tris-HCl (pH 7.4) buffer solution was used to maintain the solution pH. A 15 μmol·L⁻¹ HSA stock solution was prepared in Tris-HCl buffer solution and stored in the dark at 4°C. Dilutions of the HSA stock with Tris-HCl buffer solution were prepared immediately before use. A 1.0 mol·L⁻¹ NaCl solution was used to maintain an ionic strength of 0.1 M. A 1.0 mmol·L⁻¹ patulin solution was prepared in double-distilled water. All other reagents were of analytical grade, and double-distilled water was used throughout all experiments.

2.2. Apparatuses and Methods

2.2.1. Steady-State and Synchronous Fluorescence Spectroscopy

Steady-state fluorescence spectra were obtained using an F-4500 fluorescence spectrometer (Hitachi, Japan). The excitation and emission slit widths were 5 nm. An excitation wavelength of 295 nm and emission wavelengths between 300 and 500 nm were recorded.

The interactions between patulin and HSA were measured by the fluorescence method. The appropriate concentrations of HSA, NaCl, and patulin—15 μmol·L⁻¹, 1.0 mol·L⁻¹, and 1.0 mmol·L⁻¹, respectively—were added to a 10 mL volumetric flask; next, the mixture was diluted to graduation with Tris-HCl buffer solution. All experiments were performed at 288, 300, and 310 K. The method of synchronous fluorescence spectroscopy was carried out as described above.

2.2.2. Time-Resolved Fluorescence Spectroscopy

Time-resolved fluorescence spectra were measured by steady-state spectroscopy (FLS-920) (Edinburgh Instruments) using a standard time-correlated and single-photon counting scheme. Samples were excited with a subnanosecond pulsed diode laser at a repetition rate of 10 MHz at 295 nm. Fluorescence spectra were detected three times at 345 nm and at 288 K. The decay of the fluorescence intensity was determined with the instrument-specific software based on tail fitting. The multiexponential values were assessed by considering the reduced chi-square value (χ² < 1.10) and the random distribution of the weighted residuals near zero.

2.2.3. UV-Vis Absorption Spectra

Absorption spectra were obtained with a UV-2450 UV-Vis spectrometer (Shimadzu, Japan) at 288 K in the range of 200–500 nm using a 1 cm quartz cell. The method employed was the same as that described in Section 2.2.1.

2.2.4. CD Spectra

CD measurements were collected with a JASCO J-810 circular dichroism spectrometer (Japan) at 288 K using a 0.1 cm quartz cell. The HSA concentration was 1.5 μmol·L⁻¹, and the scanning speed was 200 nm min⁻¹. The buffer solution was used as a blank and was automatically subtracted from the samples after scanning. Each sample was measured three times at a bandwidth of 1.0 nm. The CD results were expressed in units of millidegrees.

2.2.5. Atomic Force Microscopy

AFM was carried out with a MultiMode Nanoscope IIIa (USA) equipped with a normal NP probe. The spring constant of the cantilever was 0.32 N/m, and the typical imaging resonance frequency of the fluid was 7–9 kHz. All of the samples were imaged in fluid contact mode with an O-ring liquid cell. Samples were prepared as follows: free HSA with 30 μL of 1.5 μmol·L⁻¹ HSA was added to a mica substrate and incubated for 10 min at 288 K before washing with water; HSA-patulin complexes with free HSA samples were prepared as described in step prior to adding 20 μL of a 15 μmol·L⁻¹ patulin solution, incubating for 15 min, washing with water, drying under N₂ for 4 min, and imaging in air.

2.2.6. Molecular Docking

The 3D structure of the ligand was constructed with standard bond lengths and bond angles using the molecular modeling software program SYBYL8.0 (Tripos Inc., St. Louis, USA) for Linux. Geometry optimization was performed using the standard Tripos forcefield [33] with a distance-dependent dielectric function and an energy gradient of 0.001 kcal/mol. Gasteiger-Hückel charges [34] were used.

Molecular docking was implemented using MOE2009 for Windows (Chemical Computing Group Inc., Montreal, Canada). The available X-ray structure of HSA complexed with R-warfarin (PDB code: 1H9Z) was applied in this work as the receptor. Hydrogen atoms were added to the PDB file. Then, the 1H9Z complex was handled in LigX (a module of the MOE software) to meet the docking requirements. The conformer with the lowest value was used for further analysis.

3. Results and Discussion

3.1. Analysis of Fluorescence Quenching of HSA by Patulin

The intrinsic fluorescence of HSA is derived mainly from tryptophan (Trp), tyrosine (Tyr), and phenylalanine (Phe) residues. Phe residue fluorescence has a very low quantum yield, and Tyr residue fluorescence is nearly quenched when the residue is ionized or near an amino or carboxyl group of Trp. The only tryptophan residue (Trp-214) in HSA is located in domain II, Site I. The fluorescence of Trp-214 is sensitive to the ligand to which the residue binds. Therefore, Trp-214 is often used as a probe to investigate the interaction of small ligands with HSA. Figure 2(a) shows the fluorescence spectra of HSA with different patulin concentrations at 295 nm. The maximum emission wavelength () of free HSA was 345 nm. Its intensity gradually decreased with the concentration of patulin, and the peak position was slightly blue shifted. This result indicates that patulin could quench the intrinsic fluorescence of HSA and that Trp-214 was more polar and hydrophobic after the addition of patulin.

(a)

(b)

Synchronous fluorescence is a very useful tool for investigating the microenvironments of fluorophore functional groups. According to Miller [35], the fluorescence of HSA with a () of 60 nm is characteristic of the alteration of the polarity of the microenvironment surrounding Trp-214 residues. The effect of patulin on synchronous fluorescence spectra is illustrated in Figure 2(b). The fluorescence intensity of Trp residues decreased with an increase in patulin concentration. The results correspond to those shown in the fluorescence spectra of Figure 2(a), suggesting that the microenvironment of Trp-214 was made more hydrophobic.

To further confirm the quenching mechanism, the fluorescence quenching data were analyzed with the Stern-Volmer equation: where and are the fluorescence intensity in the absence and presence of a quencher, respectively, and is the quencher concentration. is the Stern-Volmer quenching constant. The values at different temperatures are listed in Table 1. According to the fluorescence quenching mechanisms, a higher temperature would generally result in faster diffusion and the dissociation of weakly bound complexes [36]. The values increased with increasing temperature, which suggests that a dynamic quenching mechanism occurred between HSA and patulin.

Time-resolved fluorescence spectroscopy is a tool that can be used to investigate the interaction between ligands and proteins. The fluorescence lifetime can be used to directly differentiate between dynamic and static quenching. The lifetime of static quenching does not depend on the quencher concentration (i.e., ) [37, 38]. The time-resolved fluorescence spectra of the free HSA and patulin-HSA complexes are shown in Figure 3, and the fluorescence decay parameters are listed in Table 2. The fluorescence decay of the unquenched Trp-214 was biexponential (χ² = 1.007) (with = 3.06 ns [ (fraction) = 0.64], = 7.80 ns [ (fraction) = 0.36], and = 5.37 ns). These results are in agreement with those obtained for Trp-214 by Helms et al. [39]. As indicated in Table 2, the average fluorescence lifetime of Trp-214 decreased slightly with increasing patulin concentration. Therefore, these results suggest that the HSA-patulin quenching mechanism was dynamic.

3.2. The Binding Constant and Binding Site

The apparent binding constant () and the binding site number () for the patulin-HSA complex were calculated by the following equation: where, and indicate the fluorescence intensity of the system in the absence and presence of a quencher and is the total quencher concentration. The values of and for patulin-HSA are also listed in Table 1. The values increased with temperature, which indicates that the patulin-HSA quenching mechanism was dynamic. This result agrees with the results described in Section 3.1.

3.3. Binding Mode

There are several types of noncovalent interaction modes between proteins and ligands, such as hydrogen bonds, van der Waals forces, hydrophobic interaction forces, and electrostatic forces [40]. The thermodynamic parameters, enthalpy change (), and entropy change () of reaction are important for confirming what binding mode is active. Therefore, the temperature dependence of the binding constant was studied. and were obtained using the van’t Hoff equations [(3) and (4)]: where is the binding constant obtained from (1) and is the universal gas constant. and were obtained from (4). Then, the free energy change () was estimated using

The , , and values are also listed in Table 1. The and values of patulin-HSA were 8.06 kJ mol⁻¹ and 106.0 J mol⁻¹ K⁻¹, respectively. According to the results of Timasheff and Subramanian regarding various protein interactions [41, 42], a positive value is frequently regarded as evidence of a hydrophobic ligand-protein interaction considering the theory of the structure of water molecules. Thus, the hydrophobic interaction played a major role in the binding of patulin and HSA.

3.4. Energy Transfer between HSA and Patulin

The molecular distance between HSA and patulin can be determined using the Förster energy transfer theory. The overlap of patulin’s UV absorption spectrum with its fluorescence spectrum is shown in Figure 4. Based on the Förster energy transfer theory, the distance can be calculated using where is the efficiency of the transfer between HSA and patulin. and are the fluorescence intensities of HSA before and after the addition of patulin, respectively. is the distance between patulin and HSA, and is the critical distance at which the transfer efficiency is 50% [30]. The value of is calculated using where is the spatial orientation factor of the dipole, is the refractive index of the medium, and is the fluorescence quantum yield of HSA in the absence of an acceptor. In addition, is the overlap integral of the HSA and patulin fluorescence spectra. The value of is calculated using where denotes the fluorescence intensity of either donor at wavelength , and denotesthe molar absorption coefficient of patulin at wavelength (cm mol⁻¹). In this study, the value of was 1.896 × 10⁻¹⁵· cm³·L·mol⁻¹ and the value of was 0.0803. For HSA, the is equal to 2/3 and the is equal to 0.118 for an value of 1.336. Thus, was 1.896 nm, and was equal to 2.847 nm. Clearly, the distance between HSA and patulin was less than 8 nm and within . This result is in accordance with the Förster energy transfer theory and indicates that energy transfer occurred between patulin and HSA.

3.5. Effect of Patulin on the Secondary Structure of HSA

3.5.1. UV-Vis Results

Absorption at approximately 210 nm is indicative of the a-helix structure of HSA. Figure 5 shows the UV absorption spectra of HSA in the absence and presence of patulin. Figure 5 shows that HSA exhibited strong absorbance at 209 nm and weak absorbance at 280 nm. The intensities of these two absorbance peaks increased with the addition of patulin, and there was little shift wavelengths. These two results clearly indicate that there was an interaction between patulin and HSA.

3.5.2. CD Results

CD spectroscopy is a quantitative technique that is used to study the conformation of proteins in aqueous solutions. The CD spectra of HSA exhibited two negative bands at 208 and 219 nm, which characterize the α-helical structure of the protein [23]. The CD spectra of the free HSA and HSA-patulin complexes are shown in Figure 6. The secondary structure of HSA was calculated using SELCON3 (http://dichroweb.cryst.bbk.ac.uk/html); the results are listed in Table 3.

Table 3 shows that the free HSA had a high α-helix content of 55.3% and contained 8.7% β-sheets, 15.3% β-turns, and 20.7% random coils. With patulin addition, the band intensity increased at all wavelengths and no significant peak shifts were observed; furthermore, the α-helix content of HSA decreased to 50.7%, accompanied by an increase in the contents of β-sheets and β-turns to 10.6% and 17.4%. The content of random coils was only slightly altered when the molar concentration ratio of patulin to HSA was increased from 0 : 1 to 2 : 1. Thus, the binding of HSA with patulin caused conformational changes in HSA and the loss of α-helix stability.

3.5.3. The Interactions between Patulin and HSA Based on Atomic Force Microscopy

To study the changes in HSA topography with the addition of patulin, the free HSA and HAS-patulin complexes were imaged by AFM in triplicate. Figure 7 shows the AFM results obtained for the free HSA and its complexes.

(a)

(b)

As shown in Figure 7(a), HSA was adsorbed evenly on the mica surfaces. The mean height of the individual HSA molecules was nm. These dimensions are consistent with the results of previous AFM studies [43]. After the addition of patulin, the HSA molecule became swollen, and the mean height of HSA reached nm (Figure 7(b)). The aggregation of the HSA molecules is also shown in Figure 7(b). The microenvironment around the HSA became more hydrophobic after interacting with patulin. To minimize any factors adversely affecting the formation of a stable structure, the HSA molecule reduced its surface area of contact with water by molecular aggregation. These results reveal that a hydrophobic interaction between HSA and patulin may occur.

3.6. Molecular Modeling

Crystal structure analyses indicated that HSA contains the three following domains, which are structurally similar (I–III): I (residues 1–195), II (196–383), and III (384–585). The principal ligand binding sites on HSA are located in the hydrophobic cavities in subdomains IIA and IIIA, which correspond to sites I and II (according to the terminology of Sudlow et al.) [44]. Site I of HSA, which is a preferred binding pocket within the IIA subdomain [44, 45], shows affinity for warfarin, phenylbutazone, and other drugs. In addition, site II shows affinity for ibuprofen, flufenamic acid, and other ligands. To obtain more information about the patulin-HSA binding sites, molecular docking was used to simulate the patulin-HSA interaction. Figure 8 shows the patulin-HSA interaction mode. Figure 8(b) is a projection of Figure 8(a).

(a)

(b)

As shown in Figure 8, the patulin molecule was located within the binding pocket of site I (IIA), and the two rings were coplanar. The patulin molecule was inserted in the hydrophobic cavity that was formed by Ala291, Leu238, and Leu219. In addition, the pyran ring oxygen and 4-hydroxyl formed two hydrogen bonds with Arg222, and a furan ring carbonyl oxygen formed a hydrogen bond with His242. The docking results indicate that the interaction between patulin and HSA was dominated by hydrophobic forces accompanying with hydrogen bonds. In addition, several polar residues were observed near the patulin molecule, which played a subordinate role in stabilizing the ligand molecule through electrostatic interactions. For patulin-HSA, the calculated binding energy was −26.68 kJ mol⁻¹, which is near the experimental value [−22.46 kJ mol⁻¹ at 288 K], which further conformed the experimental results and demonstrated that the spontaneous binding between patulin and HSA occurred.

4. Conclusions

In this study, the interactions of patulin with HSA were investigated under simulated physiological conditions using different spectroscopic methods: AFM and molecular modeling. Steady-state and time-resolved fluorescence spectra suggest that a dynamic quenching mechanism occurred in patulin-HSA complexes. The binding parameters for the reaction were determined using the Stern-Volmer equation. The thermodynamic parameters obtained at different temperatures and the molecular modeling results indicate that hydrophobic interaction was the dominant binding force and also suggest the formation of hydrogen bonds between patulin and HSA. This finding is expected to elucidate the toxigenicity of patulin when it is combined with the biomolecular function effect, transmembrane transport, toxicological testing, and other experiments.

Abbreviations

PMTDI:	The provisional maximum tolerable daily intake
NOEL:	A no-observed-effect level
HSA:	Human serum albumin
CD:	Circular dichroism
AFM:	Atomic force microscopy
Trp:	Tryptophan
Tyr:	Tyrosine
Phe:	Phenylalanine.

Conflict of Interests

The authors declare that they have no conflict of interests.

Authors’ Contribution

Li Yuqin conceived and designed the study, carried out atomic force microscopy and data analysis, interpreted the entire results, and drafted the paper. You Guirong carried out steady-state fluorescence spectra and data analysis. Yang Zhen carried out UV-Vis spectroscopy and helped to draft the paper. Liu Caihong carried out time-resolved fluorescence spectra and data analysis. Jia Baoxiu carried out circular dichroism spectra and data analysis. Chen Jiao carried out molecular modeling and data analysis. Guo Yurong participated in the design of the study and interpreted the results. All authors read and approved the final paper.

Acknowledgment

This work was supported by the China Agriculture Research System (Cars-28).

References

O. Puel, P. Galtier, and I. P. Oswald, “Biosynthesis and toxicological effects of patulin,” Toxins, vol. 2, no. 4, pp. 613–631, 2010.
View at: Publisher Site | Google Scholar
H. M. Gashlan, “High performance liquid chromatographic determination of patulin in apple juice: investigation of its contamination levels in Saudi Arabia,” Scientific Research and Essays, vol. 4, no. 2, pp. 69–72, 2009.
View at: Google Scholar
K. Baert, F. Devlieghere, H. Flyps et al., “Influence of storage conditions of apples on growth and patulin production by Penicillium expansum,” International Journal of Food Microbiology, vol. 119, no. 3, pp. 170–181, 2007.
View at: Publisher Site | Google Scholar
M. O. Moss, “Fungi, quality and safety issues in fresh fruits and vegetables,” Journal of Applied Microbiology, vol. 104, no. 5, pp. 1239–1243, 2008.
View at: Publisher Site | Google Scholar
H. Morales, S. Marín, X. Centelles, A. J. Ramos, and V. Sanchis, “Cold and ambient deck storage prior to processing as a critical control point for patulin accumulation,” International Journal of Food Microbiology, vol. 116, no. 2, pp. 260–265, 2007.
View at: Publisher Site | Google Scholar
JECFA, Joint FAO/WHO Expert Committee on Food Additives Contaminants, WHO Food Additives Series, Toxicological Evaluation of Certain Food Additives and Contaminants, 1966.
FAO-WHO, Evalution of Certain Food Additives and Contaminants, vol. 896 of World Health Organization Technical Report Series, 2000.
U. Galvalisi, S. Lupo, J. Piccini, and L. Bettucci, “Penicillium species present in Uruguayan salami,” Revista Argentina de Microbiologia, vol. 44, no. 1, pp. 36–42, 2012.
View at: Google Scholar
C. Behm, W. Föllmann, and G. H. Degen, “Cytotoxic potency of mycotoxins in cultures of v79 lung fibroblast cells,” Journal of Toxicology and Environmental Health A: Current Issues, vol. 75, no. 19-20, pp. 1226–1231, 2012.
View at: Publisher Site | Google Scholar
R. E. Dailey, A. M. Blaschka, and E. A. Brouwer, “Absorption, distribution, and excretion of [¹⁴C]patulin by rats,” Journal of Toxicology and Environmental Health, vol. 3, no. 3, pp. 479–489, 1977.
View at: Publisher Site | Google Scholar
J. L. Richard, “Some major mycotoxins and their mycotoxicosesan overview,” International Journal of Food Microbiology, vol. 119, no. 1-2, pp. 3–10, 2007.
View at: Google Scholar
T.-S. Wu, J.-J. Yang, F.-Y. Yu, and B.-H. Liu, “Evaluation of nephrotoxic effects of mycotoxins, citrinin and patulin, on zebrafish (Danio rerio) embryos,” Food and Chemical Toxicology, vol. 50, no. 12, pp. 4398–4404, 2012.
View at: Publisher Site | Google Scholar
R. Ito, H. Yamazaki, K. Inoue, Y. Yoshimura, M. Kawaguchi, and H. Nakazawa, “Development of liquid chromatography-electrospray mass spectrometry for the determination of patulin in apple juice: Investigation of its contamination in Japan,” Journal of Agricultural and Food Chemistry, vol. 52, no. 25, pp. 7464–7468, 2004.
View at: Publisher Site | Google Scholar
N. Glaser and H. Stopper, “Patulin: mechanism of genotoxicity,” Food and Chemical Toxicology, vol. 50, no. 5, pp. 1796–1801, 2012.
View at: Publisher Site | Google Scholar
S. K. Abraham, A. Eckhardt, R. G. Oli, and H. Stopper, “Analysis of in vitro chemoprevention of genotoxic damage by phytochemicals, as single agents or as combinations,” Mutation Research—Genetic Toxicology and Environmental Mutagenesis, vol. 744, no. 2, pp. 117–124, 2012.
View at: Publisher Site | Google Scholar
R. P. Sharma, “Immunotoxicity of mycotoxins,” Journal of Dairy Science, vol. 76, no. 3, pp. 892–897, 1993.
View at: Publisher Site | Google Scholar
G. Selmanoglu and E. A. Koçkaya, “Investigation of the effects of patulin on thyroid and testis, and hormone levels in growing male rats,” Food and Chemical Toxicology, vol. 42, no. 5, pp. 721–727, 2004.
View at: Publisher Site | Google Scholar
G. Selmanoǧlu, “Evaluation of the reproductive toxicity of patulin in growing male rats,” Food and Chemical Toxicology, vol. 44, no. 12, pp. 2019–2024, 2006.
View at: Publisher Site | Google Scholar
A. Divsalar, M. J. Bagheri, A. A. Saboury, H. Mansoori-Torshizi, and M. Amani, “Investigation on the interaction of newly designed anticancer Pd(II) complexes with different aliphatic tails and human serum albumin,” Journal of Physical Chemistry B, vol. 113, no. 42, pp. 14035–14042, 2009.
View at: Publisher Site | Google Scholar
D. C. Carter and J. X. Ho, “Structure of serum albumin,” Advances in Protein Chemistry, vol. 45, pp. 153–203, 1994.
View at: Publisher Site | Google Scholar
F. Ge, C. Chen, D. Liu, B. Han, X. Xiong, and S. Zhao, “Study on the interaction between theasinesin and human serum albumin by fluorescence spectroscopy,” Journal of Luminescence, vol. 130, no. 1, pp. 168–173, 2010.
View at: Publisher Site | Google Scholar
Y. Yue, X. Chen, J. Qin, and X. Yao, “A study of the binding of C.I. Direct Yellow 9 to human serum albumin using optical spectroscopy and molecular modeling,” Dyes and Pigments, vol. 79, no. 2, pp. 176–182, 2008.
View at: Publisher Site | Google Scholar
Y. Li, X. J. Yao, J. Jin, X. G. Chen, and Z. D. Hu, “Interaction of rhein with human serum albumin investigation by optical spectroscopic technique and modeling studies,” Biochimica et Biophysica Acta, vol. 1774, no. 1, pp. 51–58, 2007.
View at: Publisher Site | Google Scholar
T. O. Hushcha, A. I. Luik, and Y. N. Naboka, “Conformation changes of albumin in its interaction with physiologically active compounds as studied by quasi-elastic light scattering spectroscopy and ultrasonic method,” Talanta, vol. 53, no. 1, pp. 29–34, 2000.
View at: Publisher Site | Google Scholar
M. Purcell, J. F. Neault, T. Malonga, H. Arakawa, R. Carpentier, and H. A. Tajmir-Riahi, “Interactions of atrazine and 2,4-D with human serum albumin studied by gel and capillary electrophoresis, and FTIR spectroscopy,” Biochimica et Biophysica Acta—Protein Structure and Molecular Enzymology, vol. 1548, no. 1, pp. 129–138, 2001.
View at: Publisher Site | Google Scholar
V. Berger, A. Gabriel, T. Sergent, A. Trouet, Y. Larondelle, and Y. Schneider, “Interaction of ochratoxin A with human intestinal Caco-2 cells: possible implication of a multidrug resistance-associated protein MRP2,” Toxicology Letters, vol. 140-141, pp. 465–476, 2003.
View at: Publisher Site | Google Scholar
D. Silva, C. M. Cortez, J. Cunha-Bastos, and S. R. W. Louro, “Methyl parathion interaction with human and bovine serum albumin,” Toxicology Letters, vol. 147, no. 1, pp. 53–61, 2004.
View at: Publisher Site | Google Scholar
S. J. Uddin, J. A. Shilpi, G. M. M. Murshid, A. A. Rahman, S. M. Marder, and M. A. Alam, “Determination of the binding sites of arsenic on bovine serum albumin using warfarin site-I specific probe and diazepam site-II specific probe,” The Journal of Biological Sciences, vol. 4, no. 5, pp. 609–612, 2004.
View at: Google Scholar
F. Ding, W. Liu, J. Diao, and Y. Sun, “Characterization of Alizarin Red S binding sites and structural changes on human serum albumin: A biophysical study,” Journal of Hazardous Materials, vol. 186, no. 1, pp. 352–359, 2011.
View at: Publisher Site | Google Scholar
X. Xie, Z. Wang, X. Zhou, X. Wang, and X. Chen, “Study on the interaction of phthalate esters to human serum albumin by steady-state and time-resolved fluorescence and circular dichroism spectroscopy,” Journal of Hazardous Materials, vol. 192, no. 3, pp. 1291–1298, 2011.
View at: Publisher Site | Google Scholar
Y. Li, H. Wang, B. Jia et al., “Study of the interaction of deoxynivalenol with human serum albumin by spectroscopic technique and molecular modelling,” Food Additives & Contaminants A, vol. 30, no. 2, pp. 356–364, 2013.
View at: Publisher Site | Google Scholar
Y. Li, B. Jia, H. Wang et al., “The interaction of 2-mercaptobenzimidazole with human serum albumin as determined by spectroscopy, atomic force microscopy and molecular modeling,” Colloids and Surfaces B: Biointerfaces, vol. 104, pp. 311–317, 2013.
View at: Publisher Site | Google Scholar
M. Clark, R. D. Cramer, and N. V. Opdenbosch, “Validation of the general purpose tripos 5.2 forcefield,” Journal of Computational Chemistry, vol. 10, no. 8, pp. 982–1012, 1989.
View at: Google Scholar
D. Pandit, A. Fiorentino, S. Bindra, and C. A. Venanzi, “Singular value decomposition analysis of the torsional angles of dopamine reuptake inhibitor GBR 12909 analogs: Effect of force field and charges,” Journal of Molecular Modeling, vol. 17, no. 6, pp. 1343–1351, 2011.
View at: Publisher Site | Google Scholar
J. N. Miller, “Recent advances in molecular luminescence analysis,” Proceedings of the Analytical Division of the Chemical Society, vol. 16, no. 3, pp. 203–208, 1979.
View at: Google Scholar
H. M. Zhang, T. T. Chen, Q. H. Zhou, and Y. Q. Wang, “Binding of caffeine, theophylline, and theobromine with human serum albumin: a spectroscopic study,” Journal of Molecular Structure, vol. 938, no. 1–3, pp. 221–228, 2009.
View at: Publisher Site | Google Scholar
J. R. Lakowicz, Principles of Fluorescence Spectroscopy, Springer, New York, NY, USA, 3rd edition, 2006.
A. V. Pastukhov, L. A. Levchenko, and A. P. Sadkov, “Spectroscopic study on binding of rutin to human serum albumin,” Journal of Molecular Structure, vol. 842, no. 1–3, pp. 60–66, 2007.
View at: Publisher Site | Google Scholar
M. K. Helms, C. E. Petersen, N. V. Bhagavan, and D. M. Jameson, “Time-resolved fluorescence studies on site-directed mutants of human serum albumin,” FEBS Letters, vol. 408, no. 1, pp. 67–70, 1997.
View at: Publisher Site | Google Scholar
X. M. He and D. C. Carter, “Atomic structure and chemistry of human serum albumin,” Nature, vol. 358, no. 6383, pp. 209–215, 1992.
View at: Publisher Site | Google Scholar
S. N. Timasheff, “Thermodynamics of protein interactions,” in Proteins of Biological Fluids, H. Peeters, Ed., p. 511, Pergamon, Oxford, UK, 1972.
View at: Google Scholar
P. D. Ross and S. Subramanian, “Thermodynamics of protein association reactions: forces contributing to stability,” Biochemistry, vol. 20, no. 11, pp. 3096–3102, 1981.
View at: Publisher Site | Google Scholar
D. Kowalczyk, J.-. Marsault, and S. Slomkowski, “Analysis of in vitro chemoprevention of genotoxic damage by phytochemicals, as single agents or as combinations,” Mutation Research—Genetic Toxicology and Environmental Mutagenesis, vol. 274, no. 6, pp. 513–519, 1996.
View at: Publisher Site | Google Scholar
G. Sudlow, D. J. Birkett, and D. N. Wade, “The characterization of two specific drug binding sites on human serum albumin,” Molecular Pharmacology, vol. 11, no. 6, pp. 824–832, 1975.
View at: Google Scholar
G. Sudlow, D. J. Birkett, and D. N. Wade, “Further characterization of specific drug binding sites on human serum albumin,” Molecular Pharmacology, vol. 12, no. 6, pp. 1052–1061, 1976.
View at: Google Scholar

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Copyright © 2014 Li Yuqin et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

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