Da
Ma
a,
Zong-Cai
Tu
*ab,
Hui
Wang
a,
Lu
Zhang
b,
Na
He
a and
David Julian
McClements
*c
aState Key Laboratory of Food Science and Technology, Nanchang University, Nanchang, Jiangxi 330047, China. E-mail: tuzc_mail@aliyun.com; Fax: +86-791-8830-5938; Tel: +86-791-88121868
bCollege of Life Science, Jiangxi Normal University, Nanchang, Jiangxi 330022, China
cDepartment of Food Science, University of Massachusetts, Amherst, MA 01060, USA. E-mail: mcclements@foodsci.umass.edu; Fax: +413-545-1262; Tel: +413-545-2275
First published on 2nd December 2016
Tyrosinase is an enzyme that promotes enzymatic browning of fruits and vegetables, thereby reducing product quality. A variety of analytical tools were used to characterize the interactions between tyrosinase and a natural tyrosinase inhibitor (glycolic acid). Hydrogen/deuterium exchange coupling with mass spectrometry (HDX-MS) was used to elucidate the interaction mechanism between glycolic acid and tyrosinase. UV-visible, fluorescence and circular dichroism spectroscopy analysis indicated that glycolic acid inhibited tyrosinase activity in a mixed-type manner with an IC50 of 83 ± 14 μM. The results of these techniques suggested that glycolic acid bound to tyrosinase through hydrophobic attraction, and this interaction led to a pronounced conformational change of the enzyme molecules. HDX-MS analysis showed that the activity of tyrosinase was primarily inhibited by a structural perturbation of its active site (His 263). This study provides a comprehensive understanding of the interaction between glycolic acid and tyrosinase, which could lead to new approaches to control tyrosinase activity in foods and other products.
An improved understanding of the interaction between tyrosinases and their inhibitors would facilitate the rational discovery of new potential candidates that could be used as inhibitors. In general, a wide variety of analytical tools and approaches are needed to provide detailed information about the interactions of small molecules with enzymes. In this study, hydrogen/deuterium exchange coupling with high-resolution mass spectrometry (HDX-MS) was used to provide fundamental information about inhibitor–tyrosinase interactions. HDX-MS can provide detailed information about the nature of the binding site on the tyrosinase molecule via analysis of the location of deuterium probe labels. In particular, we focused on the utilization of HDX-MS to characterize the interactions between tyrosinase and glycolic acid. This technique has previously been shown to be particularly powerful method for studying the interactions between proteins and small molecules.6–8
Glycolic acid is found in nature as a trace component in sugarcane, beets, grapes, and other fruits.9 It has the lowest molecular weight of all alpha-hydroxy acids because it only has two carbon atoms: one carbon atom has a carboxyl group attached while the other has a hydroxyl group attached. Studies using human skin models have shown that glycolic acid and its derivatives can inhibit tyrosinase activity and browning in melanoma cells.10,11 These studies suggest that glycolic acid may also be able to inhibit tyrosinase activity in food applications, such as the inhibition of browning in fruits and vegetables. However, there is still a relatively poor understanding of the mechanism of GA inhibition of tyrosinase activity. The purpose of this study was therefore to carry out a detailed analysis of the interaction of glycolic acid with tyrosinase using a number of spectroscopic methods in combination with HDX-MS.
The kinetics of tyrosinase inhibition by glycolic acid was characterized using UV-visible absorption spectroscopy. The nature of the interaction between glycolic acid and tyrosinase was determined using fluorescence quenching. Changes in the conformation of the tyrosinase molecules resulting from their interactions with glycolic acid were determined by synchronous fluorescence and circular dichroism (CD) spectroscopy. Detailed information about the nature of the glycolic acid binding site on the tyrosine molecule was determined by HDX-MS. The results of this research enhance our understanding of the molecular basis of glycolic acid–tyrosinase interactions, as well as providing information that will be useful for identifying new tyrosinase inhibitors that could be used as anti-browning agents in food products.
![]() | (1) |
![]() | (2) |
The slope of this equation when 1/v is plotted against 1/[S] is given by
![]() | (3) |
The values of α, Ki, Km and Vmax can be derived from these equations. Here, ν is the enzyme reaction rate in the absence and presence of GA, α is the ratio of the uncompetitive inhibition constant to competitive inhibition constant. The interaction is considered to be a noncompetitive inhibition when α is equal to 1. Ki and Km are the inhibition constant and Michaelis–Menten constant, respectively. [I] and [S] are the concentrations of inhibitor and substrate, respectively.
The fluorescence quenching data were analyzed by the well-known Stern–Volmer equation:
![]() | (4) |
The association constant (ka) was estimated using the modified Stern–Volmer equation:
![]() | (5) |
Here, ka and fa are the modified Stern–Volmer association constant and the fraction respectively.
![]() | (6) |
ΔG = ΔH − TΔS | (7) |
The ka and R are the binding constant and gas constant (8.314 J mol−1 K−1) respectively, and T values were set at 298, 304, and 310 K, respectively.
Plots of remaining activity vs. [tyrosinase] at different GA concentrations are shown in Fig. 1B. These results indicate that all the plots were linear and passed through the origin, and that the slope of the lines decreased with increasing inhibitor concentration, indicating that GA reversibly inhibited tyrosinase.16 This finding is in agreement with earlier studies.17
As shown in Fig. 2A, tyrosinase displayed a strong emission peak at 342 nm when excited at 280 nm, the peak intensity of tyrosinase decreased gradually with increasing GA concentration (0 → 22 μM) without any significant shift of the wavelength of the peak maximum, indicating that GA interacts with tyrosinase and quenches its intrinsic fluorescence.11
The Stern–Volmer plots for the quenching of tyrosinase by GA (Fig. 2B) showed that it exhibited a good linear relationship from 100 to 500 μM [Q], suggesting the quenching by one of the two classic modes (static or dynamic) occurred in the formation of the GA–tyrosinase complex.23 The calculated KSV value in Table 1 positively correlated with temperature. Moreover, the corresponding Kq values at 298, 304 and 310 K were calculated to be (1.65 ± 0.05) × 109, (1.94 ± 0.06) × 109 and (2.71 ± 0.11) × 109 L mol−1 s−1, respectively, which were considerably lower than the maximum scatter collision quenching constant of various quenchers with biopolymers (2.0 × 1010 L mol−1 s−1)24 and the Kq value increased with increasing temperature. These results indicated that dynamic or collisional quenching was dominant for the GA–tyrosinase interaction.25
T(K) | K SV (L mol−1) | R | K a (×106 L mol−1) | n | R | ΔH (kJ mol−1) | ΔG (kJ mol−1) | ΔS (J mol−1 K−1) |
---|---|---|---|---|---|---|---|---|
a R is the correlation coefficient for the KSV values. b R is the correlation coefficient for the Ka values. | ||||||||
298 | 16.53 | 0.99295 | 1.07 | 2.137 | 0.9915 | 20.309 | −51.52 | 854.4 |
304 | 19.44 | 0.99361 | 5.51 | 2.284 | 0.9920 | −56.7 | ||
310 | 27.05 | 0.98926 | 25.53 | 2.406 | 0.9865 | −61.77 |
It is also important to study whether GA alters the tyrosinase microenvironment around the tyrosine (Tyr) and tryptophan (Trp) groups. Fig. 2C and D show the synchronous fluorescence intensities of tyrosinase at different GA concentrations (0 → 22 μM) when the scanning interval Δλ was fixed at 15 and 60 nm, respectively. With increasing GA concentration, the maximum emission wavelength of Tyr residue only changed slightly (Δλ = 15 nm) (Fig. 2C), which indicated that GA had little effect on the microenvironment of the Tyr residues. This is consistent with the results for the Trp residue (Δλ = 60 nm) (Fig. 2D).
The values of ΔH, ΔS and ΔG for the GA–tyrosinase interaction are presented in Table 1. The negative values of ΔG indicate that the binding process was spontaneous. The values of ΔH and ΔS were +20.3 kJ mol−1 and +0.85 kJ mol−1 K−1, respectively, suggesting that the interaction was exothermic and mainly enthalpy favored. These thermodynamic values suggest that hydrophobic forces play an important role in the interaction between GA and tyrosinase.26
![]() | ||
Fig. 3 The CD spectra of tyrosinase in the presence of increasing amounts of GA. c (tyrosinase) = 2.4 μM, the molar ratios of GA to tyrosinase were 0![]() ![]() ![]() ![]() ![]() ![]() |
Molar ratio [GA]![]() ![]() |
α-Helix (%) | β-Sheet (%) | β-Turn (%) | Random coil (%) |
---|---|---|---|---|
0![]() ![]() |
33.9 | 18.6 | 22.4 | 25.1 |
1![]() ![]() |
26.7 | 21.4 | 23.2 | 28.7 |
1![]() ![]() |
18.6 | 26.2 | 22.5 | 32.7 |
1![]() ![]() |
19.1 | 25.4 | 21.7 | 33.8 |
8![]() ![]() |
20.5 | 24.7 | 22.4 | 32.4 |
32![]() ![]() |
19.7 | 23.4 | 22.5 | 34.4 |
Peptide location | m/z | [M + H]+ | Sequence | ||
---|---|---|---|---|---|
Observed | Theory | Error (ppm) | |||
2–8 | 808.4255 | 808.4255 | 808.4240 | 0.0015 | (M)SDKKSLM(P) |
17–31 | 1830.0617 | 1830.0617 | 1830.0596 | 0.0021 | (E) IKNRLNILDFVKNDK(F) |
47–71 | 1409.1634+2 | 2817.3195 | 2817.3155 | 0.004 | (R) DQSDYSSFFQLGGIHGLPYTEWAKA(Q) |
54–83 | 1165.2562+3 | 3493.754 | 3493.7514 | 0.0026 | (S)FFQLGGIHGLPYTEWAKAQPQLHLYKANYC(T) |
86–90 | 536.3092 | 536.3092 | 536.3079 | 0.0013 | (H) GTVLF(P) |
90–100 | 1394.6483 | 1394.6483 | 1394.6488 | −0.0005 | (L) FPTWHRAYEST(W) |
97–116 | 1187.0607+2 | 2373.1141 | 2373.1146 | −0.0005 | (L) FPTWHRAYEST(W) |
104–113 | 1018.5180 | 1018.5180 | 1018.5204 | −0.0024 | (Q) TLWEAAGTVA(Q) |
119–124 | 735.2955 | 735.2955 | 735.2944 | 0.0011 | (T) SDQAEW(I) |
124–130 | 876.4654 | 876.4654 | 876.4668 | −0.0012 | (E) WIQAAKD(L) |
145–163 | 1114.6025+2 | 2228.1977 | 2228.2001 | −0.0024 | (D) PDFIGLPDQVIRDKQVEIT(D) |
172–176 | 571.3096 | 571.3096 | 571.3086 | 0.001 | (E) VENPI(L) |
185–199 | 894.3828+2 | 1787.7583 | 1787.7581 | 0.0002 | (I)EPTFEGDFAQWQTTM(R) |
195–206 | 799.3980+2 | 1597.7887 | 1597.7871 | 0.0016 | (Q) WQTTMRYPDVQK(Q) |
206–211 | 760.3834 | 760.3834 | 760.3836 | −0.0002 | (Q) KQENIE(G) |
216–256 | 907.8537+5 | 4535.2394 | 4535.2353 | 0.0041 | (A) GIKAAAPGFREWTFNMLTKNYTWELFSNHGAVVGAHANSLE(M) |
256–263 | 966.4443 | 966.4443 | 966.4462 | −0.0019 | (L) EMVHNTVH(F) |
262–279 | 661.6978+3 | 1983.0788 | 1983.0811 | −0.0023 | (T)VHFLIGRDPTLDPLVPGH(M) |
307–319 | 768.8197+2 | 1536.6321 | 1536.6345 | −0.0024 | (W) QTMNYDVYVSEGM(N) |
330–335 | 646.3411 | 646.3411 | 646.3406 | 0.0005 | (P) GQVLTE(D) |
361–366 | 683.3416 | 683.3416 | 683.3399 | 0.0017 | (T) LGFSYP(D) |
366–378 | 738.3725+2 | 1475.7377 | 1475.7377 | 0 | (Y) PDFDPVKGKSKEE(K) |
375–390 | 1000.0034+2 | 1998.9995 | 1999.0032 | −0.0037 | (K) SKEEKSVYINDWVHKH(Y) |
392–421 | 1132.5691+3 | 3395.6927 | 3395.6979 | −0.0052 | (Y)GFVTTQTENPALRLLSSFQRAKSDHETQYA(L) |
398–405 | 913.5121 | 913.5121 | 913.5102 | 0.0019 | (Q) TENPALRL(L) |
405–431 | 1076.2021+3 | 3226.5917 | 3226.5963 | −0.0046 | (R) LLSSFQRAKSDHETQYALYDWVIHATF(R) |
428–445 | 1143.0573+2 | 2285.1073 | 2285.1026 | 0.0047 | (I) HATFRYYELNNSFSIIFY(F) |
478–483 | 646.3421 | 646.3421 | 646.3406 | 0.0015 | (R) SQDLIA(E) |
484–497 | 821.8834+2 | 1642.7595 | 1642.7570 | 0.0025 | (A) EGFVHLNYYIGCDI(G) |
496–523 | 1108.2313+3 | 3322.6793 | 3322.6815 | −0.0022 | (C) DIGQHADHEDDAVPLYEPTRVKEYLKKR(K) |
529–534 | 561.2891 | 561.2891 | 561.2879 | 0.0012 | (K) VVSAEG(E) |
531–536 | 605.2789 | 605.2789 | 605.2777 | 0.0012 | (V) SAEGEL(T) |
545–550 | 683.3416 | 683.3416 | 683.3399 | 0.0017 | (K) GAPYYL(P) |
Fig. 4 summarizes the ΔHDX values for all peptides corresponding to the mass differences of tyrosinase peptides in the presence and absence of GA. As illustrated in Fig. 4, peptides 47–71, 86–90, 119–124, 366–378, and 375–390 were protected from deuterium exchange in the presence of GA with decreased deuterium incorporation. Peptides 97–116, 185–199, 216–256, 256–263, and 262–279 exhibited increased deuterium incorporation in the presence of GA. Peptides 2–8, 90–100, 307–319, 361–366, 398–405, 405–431, 478–483 were not affected by the addition of this inhibitor, showing little changes in deuterium incorporation. Tyrosinase comprises four subunits (chain A, E; chain B, F; chain C, G; chain D, H), however, every subunit has similar active sites that contain two copper atoms and some specific amino acids. In this work, chain B and F (Fig. 5) were selected for study. Interestingly, the changes in deuterium incorporation were observed for most peptides in chain B, while little in chain F, suggesting GA disturbs the structure of chain B much greater than chain F. Peptides 97–116, 121–124, 191–194, 216–256, 256–263, 262–279, 366–378 and 375–390 are within α-helix structures. The amount of α-helix present was greatly changed by GA, which is consistent with the results from CD analysis.
![]() | ||
Fig. 5 Tyrosinase (PDB code 2Y9X): map of local HDX alterations in the presence of GA front (A) & side (B). Peptides are color-coded as follows: orange & blank = insignificant change in deuterium incorporation; cyan = the values of ΔHDX was negative; red = the values of ΔHDX was positive; blue = the peptide 262–279 (His 263). |
In this study, GA was shown to inhibit the catalytic activity of tyrosinase with an IC50 value of 83 ± 14 μM (determined spectrophotometrically). Data on the IC50 values of various tyrosinase inhibitors published in the literature or determined in this study can be ranked in the following order: cinnamic acid (IC50 = 7.5 mM)29 > morin (IC50 = 81 mM)15 ≈ GA (IC50 = 83 mM) > kojic acid (IC50 = 39 μM). These values indicate that GA has a similar or better inhibitory effect as many known tyrosinase inhibitors. Glycolic acid has the lowest molecular weight of the alpha-hydroxy acids and would therefore be expected to easily penetrate into the tissues of fruit and vegetables. Moreover, it can be isolated from natural plants or chemically synthesized, which means that it is commercially viable. Thus, glycolic acid would appear to be an extremely promising candidate for preventing the tyrosinase-catalyzed browning of foods.
The CD spectra suggest that there was an appreciable change in the secondary structure of the tyrosinase when the GA-to-tyrosinase ratio was increased from 0:
1 to 1
:
4 (i.e., from 0 to 0.6 μM GA), but that there was little further change in secondary structure when the GA level was increased higher (Fig. 3 and Table 2). In particular, there was a substantial decrease in the percentage of α-helix structure, and a corresponding increase in random coil structure, with little change in the percentages of β-sheet or β-turn structures. The GA levels where these changes in secondary structure were observed are appreciably lower than the IC50 value calculated for the inhibition of the catalytic activity of this enzyme, i.e., 83 μM. A possible explanation of this phenomenon is that the CD results only reflect changes in the secondary structure of the proteins (α-helix, β-sheet, β-turn, and random coil), rather than changes in their overall tertiary or quaternary structures. Thus, the addition of low levels of inhibitor (0 to 0.6 μM GA) could have caused appreciable changes in the local (α-helix) structure in certain regions of tyrosinase, without causing appreciable changes in the active site. Other studies have also reported that there may not be a strong correlation between changes in secondary structure and loss of tyrosinase activity.30 Overall, our results suggests there may have been some changes in the secondary structure of the enzyme at certain locations when low GA levels were added, without altering the characteristics of the active site.
Further insights into the conformational changes that occurred when GA interacted with tyrosinase were therefore obtained using HDX-MS. HDX-MS relies on the exchange of protein backbone amide hydrogen atoms with deuterium in solution. Backbone amide hydrogen atoms involved in weak hydrogen bonds or located at the surface of a protein can typically exchange rapidly, whereas those involved in strong hydrogen bonds or buried in the interior of the protein exchange more slowly. In this research, HDX-MS was first applied to elucidate the GA inhibition mechanism of tyrosinase. The binuclear copper binding site of tyrosinase is located at the heart of two pairs of antiparallel α-helices (α3/α4 and α10/α11, respectively), which make an angle of nearly 90° with each other.32 The ligands of the first copper ion, Cu-A, are the Nε2 atoms of His61 (end of helix α3), His85 (in the loop connecting α3 and α4), and His94 (beginning of α4). The ligands of the second copper ion, Cu-B, are the Nε2 atoms of His259, His263 (α10), and His296 (α11). The results from our HDX-MS study indicated that deuterium incorporation into tyrosinase occurred at peptides 256–263 (His263) and 262–279 (His263), which suggested that the tyrosinase active sites were disturbed by GA (Fig. 5). Since copper is known to play an important role in maintaining the activity of tyrosinase,31 it would be useful to measure its potential release from the enzyme in the presence of GA in future studies.
Characteristic peaks (peptides 256–263 and peptides 262–279) from tyrosinase were identified using a LTQ mass spectrometer (LTQ-MS) (Fig. 6). Both peptides were found in tyrosinase untreated or treated by GA. His263 is identified in peptides 256EMVHNTVH263 and 262VHFLIGRDPTLDPLVPGH279. The LTQ-MS of the peptides generated a series of b and y ions (b2–b7 and y1–y7, b2–b17 and y2–y17), which unambiguously confirmed the sequence of the peptide. Similarly, peptides 375–390 were identified by the LTQ-MS with m/z of 1000.0039+. The consecutive b and y ions ensure the positive identification of the peptide sequence. The peptides 86–90 were observed with significantly increased deuterium incorporation, suggesting that this area was disturbed by GA to a more open conformation. Phe90 is wedged between His94, His263, and His296, and so its conformational change may impact histidine side-chain conformations, therefore affecting the integrity of the copper binding sites.33 Our results indicate that dynamic or collisional quenching was the dominant mechanism for the GA–tyrosinase interaction, and the calculated thermodynamic parameters suggest that hydrophobic forces played an important role in the GA–tyrosinase interaction. The catalytic pocket of tyrosinase is known to be hydrophobic,34 and therefore GA may have interacted with tyrosinase primarily through hydrophobic attraction. It should be noted that GA is a highly hydrophilic molecule, although it does have some hydrocarbon regions that give it some amphiphilic character (Fig. 1A). The inhibition mechanism of GA on tyrosinase activity was investigated by various spectroscopic methods including ultraviolet-visible, fluorescence, and CD spectroscopy coupled with kinetic analysis and FTICR-MS. The results of our study demonstrated that (i) GA had a significant inhibitory activity on tyrosinase; (ii) GA was a mixed inhibitor that reversibly inhibited tyrosinase; (iii) GA bound to tyrosinase and caused a major change in the conformation of the enzyme; and, (iv) the tyrosinase active sites were disturbed due to GA binding. Our findings are supported by the results of molecular modeling simulations on related systems. For example, Wang et al. predicted that morin bound to the active site of tyrosinase using molecular modeling, which led to a conformational change of the tyrosinase molecule.15
Our study has shown that HDX-MS is a powerful analytical method that provides valuable information that can be used to elucidate the mechanism of interaction between tyrosinase and its inhibitors. This pratical technology could be used to screen different biological molecules to determine their effectiveness as tyrosinase inhibitors.
GA | Glycolic acid |
LA | Lactic acid |
HDX-MS | Hydrogen/deuterium exchange with mass spectrometry |
GA | Glycolic acid |
UV-vis | Ultraviolet visible spectrometer |
FL | Fluorescence spectrum |
CD | Circular dichroism spectrum |
FA | Formic acid |
PBS | Sodium phosphate buffer |
DMSO | Dimethyl sulfoxide |
FTICR MS | Fourier transform ion cyclotron mass spectrometry |
Tyr | Tyrosine |
Trp | Tryptophan |
Footnote |
† Electronic supplementary information (ESI) available. See DOI: 10.1039/c6fo01384h |
This journal is © The Royal Society of Chemistry 2017 |