Inhibition of thiol-containing enzymes in erythrocytes of workers exposed to lead/Inhibicion de enzimas con grupos tiol en eritrocitos de trabajadores expuestos al plomo/Inhibicao das enzimas com grupos tiol em eritrocitos de trabalhadores expostos ao chumbo.
Recent epidemiological studies have reported that even at low levels lead has a graded association with several ill-health outcomes such as hypertension, developmental defects, neurological problems, cognitive impairment, kidney damage and anemia (Muntener et al., 2003; Ekong et al., 2006; Menke et al., 2006; Bemmel et al., 2011). Olewinska et al. (2010) have shown that occupational exposure to lead is associated with damage to DNA. Both DNA damage and repair appear to be modulated by interactions between environmental and genetic factors. The response to environmental factors often depends on specific genetic polymorphisms (Dusinska and Collins., 2008). One of the most studied genes that can affect the toxicity of lead codes for [delta]-aminolevulinic acid dehydratase ([delta]-ALAD). This enzyme is the second one in the heme biosynthetic pathway and plays a role in the pathogenesis of lead poisoning (Onalaja et al., 2000). When [delta]-ALAD activity is deficient, due to lead poisoning, erythrocyte synthesis is inhibited and blood hemoglobin concentration falls. In the second step of heme synthesis, [delta]-ALAD catalyzes the formation of porphobilinogen from two molecules of [delta]-aminolevulinic acid (S-ALA). [delta]-ALAD is the most sensitive enzyme to lead in the heme pathway and has a high affinity for the metal. Lead binds to the enzyme's SH group, which normally binds zinc, preventing it from binding to S-ALA (Warren et al., 1998). Because lead effectively inhibits [delta]-ALAD activity, resulting in S-ALA accumulation in blood and urine, urinary S-ALA has also been used as a biomarker for lead exposure and as a marker of early biological effects of lead (Sithisarankul et al., 1998; Warren et al., 1998; Sakai, 2000). Studies indicate that the strong affinity to amino acid thiol groups (SH) is a characteristic shared by zinc, cadmium, mercury, and lead (Valle and Ulmer., 1972; Huang et al., 2004; Nunes-Tavares et al., 2005). Of all the enzymes that are inhibited by [Pb.sup.2+] binding to active center -SH groups, it is [delta]-ALAD about which most is known (Bernard and Lauwerys, 1987).
It is also well known that the activity of some thiol-containing enzymes may be altered by thiol/disulfide exchange between the protein sulfhydryl groups and disulfides (Gilbert, 1984). Creatine kinase (CK; EC 188.8.131.52) is a thiol-containing enzyme that catalyzes the reversible transfer of the phosphoryl group from phosphocreatine to ADP, regenerating ATP. This enzyme exerts a key role in cellular energy metabolism of tissues with high energy requirements (Wallimann et al., 1992). There are distinct CK isoenzymes, which are compartmentalized specifically in places where energy is released (mitochondria) or used (cytosol) (Friedman and Perryman., 1991). Adenylate kinase (AK; EC 184.108.40.206) is a thiol-containing enzyme like [delta]-ALAD and CK, catalyzing the reversible transfer of phosphoryl between ATP and AMP (Willemoes and Kilstrup, 2005). This enzyme, along with CK, is responsible for the enzymatic phosphotransfer network; in other words, it is responsible for the transfer of the phosphate of ATP where it is produced (mitochondria) to the place where it is consumed (cytosol) (Dzeja and Terzic, 2003). Both enzymes, CK and AK, are intimately associated in such a way that when one enzyme activity is reduced, the activity of the other enzyme is enhanced (Dzeja et al., 1999, 2002). Lead affects various hematological systems, such as heme biosynthesis and catabolism of pyrimidine nucleotides. These metabolic disorders can be used as indicators for biological monitoring of lead exposure, on the basis of dose-effect relationships between blood lead concentrations (BPb) and the biochemical effects of lead. In this study, we investigated the effect of [Pb.sup.2+] on the activity of the thiol-enzymes [delta]-ALAD, CK, AK and on levels of the non-enzymatic antioxidant defense mechanism glutathione (GSH) in human erythrocytes from lead-exposed workers and demonstrate that CK activity can be used for biological monitoring of lead exposure.
Materials and Methods
We recruited 22 male lead-exposed workers 20-50 years old (mean 35 years) and 21 normal volunteers. All volunteers provided informed consent before venous blood samples were collected and treated with heparin, during their routine physical examinations. These workers were employed in manufacturing and recycling of automotive batteries in Rio Grande do Sul, Brazil. Control subjects were fifteen males 20-48 years old (mean 34 years) and six females 18-40 years old (mean 29 years) with no history of lead exposure. Controls underwent clinical blood analysis and abnormal findings were not found. Exclusion criteria were as follows: history, or current physical findings of serious cardiovascular, renal, hepatic, endocrine, metabolic or gastrointestinal diseases or previous pharmacological treatment. All subjects provided informed consent in writing and participation was voluntary. The study was approved by Feevale University Ethics Commission.
Venous blood was used for hematological testing. Blood was drawn by venous puncture and collected in EDTA tubes. The following parameters were measured using a Siemens automatic hematology system: red blood cell count (RBC), hemoglobin (HGB), hematocrit (HCT), mean corpuscular volume (MCV), mean corpuscular hemoglobin (MCH), mean corpuscular hemoglobin concentration (CHCM) and white blood cell count (WBC).
Determination of lead levels in blood
Blood lead (BPb) was quantified as follows. Samples were diluted to 1:10 with a dilution solution containing 0.1% Triton X-100 (v/v) and 1% HNO3 (v/v) in Milli-Q water. Lead was analyzed using a Perkin Elmer Analyst 600 graphite furnace atomic absorption spectrometer with a pyrolytic graphite-coated furnace and a permanent matrix modifier composed of tungsten, rhodium, and ammonium hydrogen phosphate. The injection volume was 20gl of the diluted sample. The temperatures used for the drying phase were 120[degrees]C.5 x [s.sup.-1] (rise time 10s) followed by 200[degrees]C.5 x [s.sup.-1] (rise time 5s); 600[degrees]C.20 x [s.sup.-1] (rise time 10s) for ashing; 1700[degrees]C.3 x [s.sup.-1] (step mode) for atomization; and 2200[degrees]C.4 x [s.sup.-1] (rise time 1s) for cleaning. Argon 99.999% (v/v) (White Martins, Brazil) was used as carrier gas at a flow rate of 250ml x [min.sup.-1] for all phases except atomization. The detection and quantification limits of the method employed are 0.06 and 0.15[micro]g x [dl.sup.-1], respectively.
Preparation of erythrocytes
Blood was collected by venous puncture into heparinized tubes. Each sample was centrifuged at 800g for 10min and the plasma and white cells were carefully removed by aspiration to avoid loss of erythrocytes. The packed cells were washed three further times at 700g for 5min with isotonic buffer. After this process, the erythrocytes were hemolyzed by adding distilled water at a dilution of 1:5 in a tube, then each sample was centrifuged at 800g for 10min and the supernatant was separated for biochemical analysis.
Erythrocyte CK activity
Aliquots from heparinized blood were used for determination of creatine kinase (CK) activity. CK activity was assessed in lysed erythrocytes in accordance with the preparation of erythrocytes (above). The reaction mixture contained the following final concentrations: 60mM Tris-HCl buffer, pH 7.5, 7mM phosphocreatine, 9mM MgS[O.sub.4], and ~1[micro]g protein in a final volume of 0.13ml.. After 30min of pre-incubation at 37[degrees]C, the reaction was started by the addition of 0.42[micro]mol ADP. The reaction was stopped after 10min incubation by the addition of 1 [micro]mol p-hydroxymercuribenzoic acid. The reagent concentrations and the incubation time were chosen to assure linearity of the enzymatic reaction. Appropriate controls were carried out to measure chemical hydrolysis of phosphocreatine. The creatine formed was estimated according to the colorimetric method of Hughes (1962). The color was developed by the addition of 0.1ml of 2% [alpha]-naphthol and 0.1ml 0.05% diacetyl in a final volume of 1ml and read at 540nm after 20min. Results were expressed as mmol of creatine formed per min per mg protein.
Erythrocyte [delta]-ALAD activity
[delta]-aminolevulinic acid dehydratase activity was assayed as described by Berlin and Schaller (1974). Aliquots from heparinized blood were used for determination of [delta]-ALAD activity. [delta]-ALAD activity was assessed in lysed erythrocytes in accordance with the preparation of erythrocytes (above). Modified Ehrlich's reagent was used to react with the porphobilinogen (PBG) final product to yield a pink-colored compound, which was measured at 555nm. Activity was expressed as [micro]mol PBG/ min/lit of erythrocyte.
Erythrocyte AK activity
Aliquots from heparinized blood were used for determination of adenylate kinase (AK) activity. AK activity was assessed in lysed erythrocytes. AK activity was measured with a coupled enzyme assay with hexokinase (HK) and glucose 6-phosphate dehydrogenase (G6PD), according to Oliver (1955) with the modifications introduced by Dezja et al. (1999). The reaction mixture contained 100mM KCl, 20mM HEPES, 20mM glucose, 4mM Mg[Cl.sub.2], 2mM [NADP.sup.+], 1mM EDTA, 4.5U/ml of HK, 2U/ml of G6PD and 1[micro]g of protein homogenate. The reaction was initiated by the addition of 2mM ADP and the reduction of [NADP.sup.+] was followed at 340nm for 3min in a spectrophotometer. ADP, [NADP.sup.+], G6PD and HK were dissolved in water. Reagents concentration and assay time (3min) were chosen to ensure linearity of the reaction. Results were expressed in [micro]mol of ATP formed per min per mg of protein.
Reduced GSH concentrations
Reduced glutathione (GSH) concentrations were measured according to Browne and Armstrong (2002). Erythrocytes were hemolyzed with 1[micro]l Triton X-100 and 10min later precipitated with 20% trichloroacetic acid (w/v). After centrifugation, the supernatant aliquots were diluted in 20 volumes of (1:20, v/v) 100mM sodium phosphate buffer pH 8.0, containing 5mM EDTA. Of this preparation, 100[micro]l were incubated with an equal volume of o-phthaldialdehyde (1mg/ml methanol) at room temperature during 15min. Fluorescence was measured using excitation and emission wavelengths of 350 and 420nm, respectively. A calibration curve was prepared with standard GSH (0.01-1mM) and concentrations are expressed as nmol of GSH/mg of protein.
Erythrocyte protein content was determined using the method described by Lowry and co-workers (1951), using bovine albumin as the standard.
Data were analyzed using Student's t test for independent samples. Dose-dependent effects were analyzed by linear regression. All data were analyzed using the Statistical Package for the Social Sciences (SPSS 17.0 for Windows; Leech et al., 2005).
Table I shows the results of those clinical analyses for which there was a significant difference between the individuals in the exposed and control groups. The following results were all significantly lower in lead-exposed individuals than in controls: RBC ([t.sub.(41)]=6.88, *** p < 0.0001); HGB ([t.sub.(41)]= 13.08, ** p < 0.0001); HCT ([t.sub.(41)]=5.67, ** p < 0.0001); MCH ([t.sub.(41)]=12.06, ** p < 0.0001); and MCHC ([t.sub.(41)]=2.63, * p < 0.05). There was no significant difference between the two groups in terms of WBC ([t.sub.(41)]=0.940, p=0.692) or MCV ([t.sub.(41)]=0.90, p=0.371).
As shown in Table II, blood lead concentrations were significantly higher in lead-exposed individuals than in controls ([t.sub.(41)]=-26.64, ** p < 0.0001) while CK (t(31)=2.87, ** p < 0.01) and [delta]-ALAD (t(28)=9.26, ** p < 0.0001) activities were both significantly lower in lead-exposed individuals than in controls. We also found that lead had no effect on AK activity (t(30)=1.52, p=0.24) and erythrocyte glutathione content was reduced (t(26)=3.04, ** p < 0.01) in lead-exposed individuals compared with normal volunteers. Furthermore, lead significantly inhibited CK (t=6.89, p=-0.43, * p < 0.05) and [delta]-ALAD (t= 16.71, p=-0.85, ** p < 0.0001) activities in a dose-dependent manner. Figures 1 and 2 illustrate the strength of the relationship between blood lead levels and biomarkers of lead toxicity, including CK and [delta]-ALAD activity. Figure 3 illustrates the lead dose-dependent effect analyzed by linear regression for lead-exposed individuals vs normal volunteers; the figure reveals a significant regression for CK against [delta]-ALAD activity (t= 14.71, [beta]=0.58, ** p < 0.001). These results indicate apparent dose-effect relationships between CK and [delta]-ALAD activity. Figure 4 illustrates the lead dose-dependent effect analyzed by linear regression for lead-exposed individuals vs normal volunteers. This figure illustrates a significant regression for blood lead levels against GSH content (t=2 3.51, [beta]=-0.85, p < 0.0001). Figures 5 and 6 illustrate a significant regression for CK activity against GSH content (t= 10.68, p=0.54, p < 0.01) and for [delta]-ALAD activity against GSH content (t=6.96, [beta]=0.84, p < 0.0001), respectively. These results indicate apparent dose-effect relationships between GSH content and CK activity and between GSH content and [delta]-ALAD activity.
In this study we investigated the effect of lead on the activity of the thiol-enzymes CK and [delta]-ALAD in human erythrocytes from lead-exposed workers. The values for several red-cell parameters (hemoglobin, hematocrit, red blood cell count and mean corpuscular volume) were lower in lead-exposed individuals than in controls. These results suggest that lead inhibits CK and [delta]-ALAD activity by interacting with their thiol groups. Inhibition of these enzymes and GSH depletion can induce erythrocyte cell death through hemolysis. The results indicate an apparent dose-effect relationship between GSH content and CK activity and between GSH content and [delta]-ALAD activity. Therefore, simultaneous suppression of CK and [delta]-ALAD activity could severely impair both erythrocyte metabolism and antioxidant defenses (GSH), with severe consequences for cell function and survival. Inhibition of these enzymes can induce erythrocyte cell death through hemolysis. The results indicate an apparent dose-effect relationship between BPb and CK activity and between BPb and [delta]-ALAD activity.
Lead toxicity leads to free radical damage via two separate, although related, pathways: 1) generation of reactive oxygen species (ROS), including hydroperoxides, singlet oxygen and hydrogen peroxide; and 2) direct depletion of antioxidant reserves (Ercal et al., 2011). In any biological system where ROS production increases, antioxidant reserves are depleted. One of the effects of lead exposure impacts glutathione metabolism (Lepper et al., 2010). Glutathione plays an important role in antioxidant defense and redox regulation (Wu et al., 2004). It not only reacts with free radicals, but can also form conjugates with numerous substances, including heavy metals (Meister, 1994). It is possible that the reduction in concentrations of GSH and non-protein thiols in the liver and kidneys after exposure to [Pb.sup.2+] could be the result of lead's high degree of affinity for SH groups (Gurer et al., 1999). On the other hand, it is known that GSH depletion induces cell death by apoptosis (Armstrong and Jones, 2002). Erythrocytes have a high affinity for lead, binding 99% of that present in the bloodstream. Lead has a destabilizing effect on cell membranes, and in RBC the effect is to decrease cell membrane fluidity and increase the erythrocyte hemolysis rate. Hemolysis appears to be the end result of ROS-generated lipid peroxidation in the RBC membrane (Lawton and Donaldson, 1991). Hypochromic or normochromic anemia is a hallmark of lead exposure resulting from ROS generation and subsequent erythrocyte hemolysis (Gurer and Ercal, 2000). Lead, in common with silver, mercury, and copper, is considered to be a strong hemolytic agent capable of causing erythrocyte destruction through formation of lipid peroxides in cell membranes (Farant and Wigfield, 1982).
In addition to membrane peroxidation, lead exposure causes hemoglobin oxidation, which can also cause RBC hemolysis. The mechanism responsible for this reaction is lead-induced inhibition of [delta]-ALAD. Lead's toxic effects are manifest in depressed heme formation and [delta]-ALAD is the enzyme that is most sensitive to this depression (Farant and Wigfield, 1982). Feksa et al. (2012) found that pyruvate kinase (PK) behaves similarly to [delta]-ALAD, contributing further harm to erythrocyte survival systems. Pyruvate kinase is an enzyme that catalyzes the conversion of phosphoenolpyruvate (PEP) to pyruvate, producing adenosine triphosphate (ATP) from adenosine diphosphate (ADP) (Feksa et al., 2012). Our results suggest that there is a strong correlation between inhibition of CK, [delta]-ALAD and induction of cell death by hemolysis. This is manifest in the alterations to several hematological parameters, such as HGB, HCT, RBC and MCV, which were lower in lead-exposed individuals than in controls. However, further studies to evaluate the activity of thiol-containing enzymes such as CK and [delta]-ALAD in occupationally lead-exposed workers are still needed. In this study it is shown that CK behaves similarly to [delta]-ALAD, contributing further harm to erythrocyte survival systems. The AK activity did not change in the presence of lead. We can explain this effect because both enzymes, CK and AK, which are responsible for transferring phosphate from ATP that is produced to the location where it is consumed, are intimately associated; when one enzyme activity is reduced, the activity of the other enzyme is enhanced (Dzeja et al., 1999, 2002). The adenylate kinase is responsible for the reversible conversion between phosphates of ATP, ADP and AMP (Bae and Phillips 2006). AK doubles the energy potential of ATP, having the ability of regenerate ATP from two ADP and by the regulation of processes involving adenine nucleotides (Noma, 2005; Willemoes and Kilstrup, 2005). CK has the main function in energy metabolism, where it works like a buffer system of levels of cellular ATP; it catalyzes the reversible transfer of the phosphoryl group of phosphocreatine to ADP, regenerating ATP (Warchala et al., 2006). Inhibition of CK and PK activity (Feksa et al., 2012) and no change in activity of AK in the erythrocyte can help avoid severe consequences for cell function and survival. The study of the mechanisms by which lead acts may contribute to a better understanding of the symptoms caused by this metal.
Received: 06/09/2014. Modified: 12/28/2014. Accepted: 01/06/2015.
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Thereza Luciano Trombini. Graduate in Biomedicine, Universidade Feevale (UFeevele), Brazil. Biomedical Specialist, UFeevale, Brazil.
Evandro Oliveira. Graduate in Biomedicine, UFeevale, Brazil. Biomedical Specialist, UFeevale, Brazil.
Daiane Bolzan Berlese. Doctor in Toxicological Biochemistry, Universidade Federal de Santa Maria (UFSM), Brazil. Professor, UFeevale, Brazil. Address: Grupo de Pesquisa em Bioanalise, Instituto de Ciencias da Saude, Universidade Feevale, Novo Hamburgo, RS, Brazil. e-mail: email@example.com
Renato Minozzo. Doctor in Genetics and Applied Toxicology, Universidade Luterana do Brasil. Professor, UFeevale, Brazil.
Tassia de Deus. Graduate in Biomedicine, UFeevale, Brazil. Biomedical Specialist, UFeevale, Brazil.
Cristina Deuner Muller. Graduate in Biomedicine, UFeevale, Brazil. Biomedical Specialist, UFeevale, Brazil.
Rafael Linden. Doctor in Cell and Molecular Biology, Pontificia Universidade Catolica do Rio Grande do Sul, Brazil. Professor, UFeevale, Brazil.
Vandre Casagrande Figueiredo. Master in Biology, Universidade Federal do Rio Grande do Sul (UFRGS), Brazil. Doctoral student, University of Auckland, Nova Zealanda.
Clovis Milton Duval Wannmacher. Doctor in Biology, UFRGS, Brazil. Professor, UFRGS, Brazil.
Greicy Michelle Marafiga Conterato. Doctor in Toxicological Biochemistry, UFSM, Brazil. Professor, Universidade Federal de Santa Catarina, Brazil.
Luciane Rosa Feksa. Doctor in Biology, UFRGS, Brasil. Professor, UFeevale, Brazil.
TABLE I EFFECT OF LEAD ON BLOOD WHITE CELL COUNT, RED CELL COUNT, HEMOGLOBIN, HEMATOCRIT, MEAN CORPUSCULAR VOLUME, MEAN CORPUSCULAR HEMOGLOBIN AND MEAN CORPUSCULAR HEMOGLOBIN CONCENTRATION IN 21 NORMAL VOLUNTEERS AND 22 LEAD-EXPOSED WORKERS Control Lead-exposed WBC (/[micro]l) 8010 [+ or -] 1333 7836 [+ or -] 1510 RBC (106/[micro]l) 4.59 [+ or -] 0.44 3.78 [+ or -] 0.31 *** HGB (g/dl) 14.38 [+ or -] 0.33 12.88 [+ or -] 0.41 *** HCT (%) 42.28 [+ or -] 3.5 37.0 [+ or -] 2.51 *** MCV (fl) 84.61 [+ or -] 2.63 83.86 [+ or -] 2.83 MCH (pg) 30.9 [+ or -] 1.75 25.36 [+ or -] 1.22 *** MCHC (g/dl) 34.2 [+ or -] 1.64 32.86 [+ or -] 1.78 * Data are expressed as mean [+ or -] SD. Different from controls to: *** p < 0.0001, * p < 0.05 (Student's t test). TABLE II BLOOD LEAD CONCENTRATION, A-ALAD, CK AND AK ACTIVITY IN ERYTHROCYTES FROM NORMAL VOLUNTEERS AND LEAD-EXPOSED WORKERS Control (n=12-21) Lead-exposed (n=16-22) Blood lead 1.88 [+ or -] 0.39 61.9 [+ or -] 10.3 *** concentration S-ALAD activity 29.1 [+ or -] 7.1 9.2 [+ or -] 4.7 *** CK activity 6.28 [+ or -] 1.2 5.12 [+ or -] 1.12 *** AK activity 3.68 [+ or -] 0.79 3.24 [+ or -] 0.62 GSH content 1.33 [+ or -] 0.85 0.678 [+ or -] 0.15 *** Data are expressed as mean [+ or -] SD for experiments performed in duplicate. Different from controls to: *** p < 0.0001
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|Title Annotation:||articulo en ingles|
|Author:||Trombini, Thereza Luciano; Oliveira, Evandro; Berlese, Daiane Bolzan; Minozzo, Renato; De Deus, Tass|
|Date:||Feb 1, 2015|
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