Corresponding Author: Caterina Manna and Michel Prudent
Department of Precision Medicine, School of Medicine, University of Campania “L. Vanvitelli”, Via De Crecchio 7, Naples, 80138 (Italy)
Tel. +39 0815667523, E-Mail firstname.lastname@example.org
Département Innovation et Produits Thérapeutiques, Transfusion Interrégionale CRS, Biopôle Secteur Croisettes, Bâtiment Metio, Route de la corniche 2, CH-1066 Epalinges (Switzerland)
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Effect of Mercury on Membrane Proteins, Anionic Transport and Cell Morphology in Human Erythrocytes
Rosaria Notarialea Emmanuel Längstb Pasquale Perronea David Crettazb Michel Prudentb,c,d Caterina Mannaa
aDepartment of Precision Medicine, School of Medicine, University of Campania “Luigi Vanvitelli”, Naples, Italy, bLaboratoire de Recherche sur les Produits SanguinsInnovation et Produits Thérapeutiques, Transfusion Interrégionale CRS, Epalinges, Switzerland, cCenter for Research and Innovation in Clinical Pharmaceutical Sciences, Institute of Pharmaceutical Sciences of Western Switzerland, University Hospital and University of Lausanne, Lausanne, Switzerland, dInstitute of Pharmaceutical Sciences of Western Switzerland, University of Geneva, University of Lausanne, Lausanne, Switzerland
Mercury (Hg) is a heavy metal classified as one of the most hazardous global pollutants [1, 2], exerting its toxic effects even at trace amounts. Hg contamination, indeed, is extensive in all environmental compartments such as soil, air, and water. It reacts adversely within organisms and bioaccumulates in aquatic animal tissue. The consumption of contaminated fish, indeed, represents the major Hg route of human exposure . In particular, the average blood mercury level of consumers of high-fish diets was 3.7 times higher than those observed in those who reported consuming no fish . This natural element can exist in different redox forms (elemental, inorganic and organic), each with a different pathway of exposure and a unique toxicological profile . Hg reacts with high affinity to SH groups and therefore binds a variety of cellular components, but mechanisms underlying its cytotoxicity turn out to be very complex and not yet fully understood . Overall, Hg poisoning in humans manifests as neurological, kidney, immune, and respiratory disorders, associated with imbalances in calcium homeostasis, stimulation of apoptosis, and alterations in the antioxidant defense system [7–10].
A growing body of evidence suggests that Hg exposure may lead to adverse effects on cardiovascular tissues . Several experimental evidence indicate that cardiac function is directly affected by Hg exposure. Specifically, high levels of Hg can induce alterations in heart function through dysregulation of humoral and neuronal modulation, alterations in innervation, or alterations in blood vessels, resulting in decreased cardiac excitability and contractility [12, 13]. Furthermore, there is an increasing body of data associating Hg exposure and endothelium dysfunction. In this respect, workers occupationally exposed to Hg vapor show increased blood concentration of this heavy metal, associated with significant alterations in the coagulation system . Accordingly, Hg intoxication is associated with an increased risk of cardiovascular diseases (CVD) [15–17].
Regardless of the route of absorption, Hg finds its way through blood stream allowing its distribution to tissues and organs. Among blood cells, human erythrocytes (RBC) are an important target of Hg toxicity because this metal ion preferentially accumulates in these cells, reaching concentrations higher than those found in plasma [18, 19]. Indeed, the highest blood mercury concentrations reported in humans were in gold mine workers in the Amazon area, whose blood mercury levels reached 150 μg/L (~0.75 μM), in contrast to the average plasma levels of around 83.3 μg/L (0.4 μM) [14, 20].
In recent years, particular attention has been focused on the mechanisms promoting vascular dysfunction and thrombotic events as a consequence of Hg-induced RBC damage [21, 22]. We recently reviewed the Hg-induced metabolic and morphological alterations that could affect RBC physiology, responsible for activation of a pro-thrombotic activity and likely acting as a major player in endothelial dysfunction . Among these alterations, loss of physiological membrane asymmetry, due to phosphatidylserine (PS) exposure, is proved to enhance RBC adhesion to endothelial cells and clot formation . Alterations in RBC membrane proteins, including cytoskeleton proteins and Band 3 (B3p), the most abundant integral protein on the membrane, have also been reported to be prothrombotic factors . In particular, modification of these proteins results in morphological changes and microvesicles (MVs) generation [24, 25] that are known to contribute to thrombotic events . All together, these effects design RBC as an active contributor to vascular dysfunction associated with Hg intoxication.
A preliminary study from our group indicated that Hg exposure induces RBC membrane protein alterations . To investigate Hg-induced cytotoxicity at the molecular level, the possible interaction of this heavy metal with specific membrane proteins was investigated. For this aim, human RBC were treated in vitro with different HgCl2 concentrations (range 10-40 µM) and the electrophoretic profile of membrane proteins as well as the expression levels of Ankyrin, a protein essential for membrane-cytoskeleton linkage and Flotillin-2, a major integral protein of RBC lipid rafts [28, 29], were evaluated. Furthermore, Hg-induced alterations in B3p transport function, PS-exposing MVs and RBC morphological changes were assessed.
Materials and Methods
Chemicals and solutions
DIDS (4,40-diisothiocyanato-stilbene-2, 20-disulfonate), deoxycholic acid (DC), ponceau S and HgCl2 were from Sigma Chemical Co. Bromophenol blue and Coomassie Bue Brilliant R-250 were purchased from Fluka Chemie, Buchs, Switzerland. Tween-20 was bought from Roche Diagnostics (Mannheim, Germany), PBS 10x (1x PBS eq. to 137 mM NaCl, 2.7 mM KCl, 8.1 mM Na2HPO4 and 1.8mMKH2PO4) from Laboratorium Dr. G. Bichsel (Interlaken,Switzerland), EDTA from Merck (MSD Merck Sharp & Dohme, Luzern, Switzerland), Tris-HCl from BIO-RAD (Hercules, CA, United States), ethanol from Thommen-Furler AG (Rüti bei Büren, Switzerland), SureBlock from Lubio Science (Luzern, Switzerland), BenchMark Protein Ladder (prestained or not) from Invitrogen (Carlsbad, CA, United States). Furthermore, Ankyrin B (2.20): sc-12718 and Flotillin-2 (Santa Cruz Biotechnology) as well as Annexin V-fluorescein isothiocyanate (V-FITC) Apoptosis Detection Kit (556547, BD Pharmigen, Franklin Lakes, NJ, USA) were used. DIDS was prepared in DMSO and diluted from 10 mM or 100 mM stock solution. Preparation of RBC and treatment with HgCl2Whole blood was obtained with informed consent from healthy donors at Transfusion Interrégionale CRS (Epalinges, Switzerland) and RBC concentrates were prepared using a top-bottom bag system and mixed with saline adenine glucose mannitol solution for storage, as previously described . It was collected in tubes and centrifuged at 2,000 g for 10 min at 4 °C. The RBC fraction was washed twice with isotonic saline solution (0.9 % NaCl) and resuspended in Krebs solution (pH 7.4) containing (mM) NaCl 125, KCl 4, MgSO4 1, Hepes 32, CaCl2 1, glucose 2.8, to obtain a 10 % (v/v) hematocrit (or 3% for the sulphate transport measurement). RBC were co-incubated at 37 °C for 4 h (only for sulphate transport measurement) or 24 h with HgCl2 (10, 20, 40 μM).
Preparation of erythrocyte membranes
After HgCl2 treatment, RBC were washed twice in 0.9 % NaCl (2 v) and centrifuged at 2,000 g for 10 min at 4 °C. Samples were lysed by incubation for 1 h at 4 °C in a hypotonic solution of 0.1x PBS under agitation (4 v of 0.1x PBS per 1 v of RBC pellet).
Membranes were separated by ultracentrifugation at 21,500 g, 75 min, 4 °C, to separate intracellular contents from membranes. We separated the supernatant, which contains the cytosolic fraction, from the lower part containing the membranes. The latter was washed 8 times (centrifugation at 21,500 g, 30 min, 4 °C) to remove as much as possible hemoglobin (Hb) from membranes. RBC membranes were stored at -80 °C until protein extraction .
Thawed samples were centrifuged (21,500 g, 30 min, 4 °C). Subsequently, total membrane proteins were extracted under native conditions from pelleted membranes with DC buffer: 1 % DC in 50 mM Tris-HCl, 150 mM NaCl, pH 8.1. A final centrifugation was performed at 21,500 g, 30 min, 4 °C. Protein concentration of the supernatant, containing membrane proteins and cytoskeleton and were quantified using a nanodrop 2000c (Thermo scientific) .
Total membrane protein extracts were analyzed by SDS-PAGE. Ten μg of proteins from each sample and 3 µL of BenchMark Protein Ladder (or 10 µL of BenchMark Prestained Protein Ladder for Western blot, WB) were loaded on gels (Mini- PROTEAN TGX gels, 4–15%, BIO-RAD, United States). Following separation, proteins were stained with Coomassie Brilliant Blue R250 and acquired using a GelDoc system via Quantity One v.4.4.0 software (BIO-RAD, Hercules, CA, USA). The densitometric analysis of gel bands was carried out using the software ImageJ (Rasband, W.S.,ImageJ, U.S. National Institute of Health, Bethesda, Maryland, USA, https://imagej.nih.gov/).
The WB analyses were performed on PVDF membranes (transfer 1 h at 100 V in Tris-Glycine buffer inside a Mini Trans-Blot Electrophoretic Transfer cell).
Membranes were rinsed in TBS-T (1x TBS, 0.05 % Tween-20) and blocked with SureBlock buffer (4 % in TBS-T) during 1 h at RT under agitation. Then, the membranes were washed 3 x 5 min in TBS-T. Blots were incubated overnight at 4 °C under agitation with the primary antibody (Ankyrin B 1/200 and Flotillin-2 1/6,000 in SureBlock buffer). After a quick rinse and washes of 3 x 5 min at RT in TBS-T, the membranes were re-incubated in SureBlock buffer for 30 min at RT under agitation.
Subsequently, membranes were incubated with the secondary antibody (Polyclonal goat anti-mouse immunoglobulins HRP, Dako, Denmark) diluted at 1/10,000 in SureBlock buffer, for 1 h at RT under agitation. The membranes were finally washed several times in TBS-T at RT under agitation.
The ECL reaction was achieved using the ECL Western blotting detection reagents (GE Healthcare, Little Chalfont, Buckinghamshire, United Kingdom) 1 min and the images were acquired by means of ImageQuant LAS 500 (GE healthcare, Uppsala, Sweden).
After the ECL reaction, the blots were rinsed and washed 3 x 5 min in TBS-T and then stripped for 40 min at RT under agitation in 20 mL of RestoreTM Western Blot Stripping Buffer (Thermo Scientific, Rockford, IL, United States). Then, the blots were rinsed and washed again 3 x 5 min in TBS-T before a new blocking for 20 min at RT under agitation in SureBlock buffer. Finally, they were rinsed, washed 2 x 5 min in TBS-T and stored at 4 °C for further immunodetection Bands of interest were quantified by densitometry of the ImageJ software (1.51w1) and expressed as “volume”. The data were then corrected by the total protein loading detected on Ponceau S by densitometry. The relative volumes were calculated as follows:
Relative VolumeProtein = VolumeProtein,ECL / VolumeWhole proteins,Ponceau ,
where VolumeProtein,ECL is the band volume of the protein of interest from WB and VolumeWhole proteins,Ponceau is the amount of loaded proteins determined by the densitometry analyses of whole lane from Ponceau red-stained membrane .
Sulphate transport measurement
According to Romano and Passow , samples were suspended in an isotonic medium (in mM: 118 Na2SO4, 10 HEPES, 5 glucose, pH 7.4) at a hematocrit of 3%, and centrifuged for 5 minutes at 1,000g. After 15, 30, 45 and 60 minutes of incubation at 37 °C with or without (control) HgCl2 (10-40 µM), 5μM of DIDS stopping medium was added at different intervals to 500 µL of samples and kept on ice. The presence of DIDS, a compound that binds irreversibly and specifically to the extracellular moiety of the integral membrane B3p, inhibits SO42- transport in RBC .
After the last sample withdrawal, RBC were washed two times in cold isotonic solution (in mM: 150 NaCl, 20 HEPES, pH 7.4) at 4 °C, 1000 g, 5 min to remove SO42- from the external medium and hemolyzed in 1 mL of distilled water, while proteins were hydrolyzed by perchloric acid (4 % v/v).
The membranes were then discarded by pelleting them with a 10 min centrifugation at 4,000 g at 4 °C. Sulphate ions in the supernatant were precipitated by sequentially adding and mixing 1 mL of a glycerol-distilled-water solution (1:1), 1 mL of a NaCl-HCl (4 M and 37%, respectively) solution (12:1) and 500 µL of 1.24 M BaCl2 x 2H2O, to obtain a homogeneous barium sulphate precipitate. The intracellular sulphate concentration was measured by atomic absorption spectrophotometry at 425 nm. According to Remigante et al. , in order to convert the absorption to [SO42−] L cells × 10−2, a calibrated standard curve previously obtained by precipitating known SO42− concentrations was used. Furthermore, the rate constant (min−1) was calculated by the equation: Ct = C∞ (1 − e−rt) + C0, where Ct, C∞, and C0 represent the intracellular SO42− concentrations, respectively, at time t, 0, and ∞; e is the Neper number (2.7182818); r is the rate constant accounting for the process velocity, and t is the time fixed for each sample withdrawal. The rate constant is the time needed to reach 63% of total SO42− intracellular concentration and [SO42−] L cells × 10−2 reported in figure stands for SO42− micromolar concentration trapped by 10 mL erythrocytes (3% hematocrit).
Quantification assay of MVs by flow cytometry
In this study, we measured MVs-annexin V-positive to evaluate the PS-exposure. MVs were obtained from intact RBC after treatment with HgCl2. RBC were centrifuged at 2,000 g during 10 min at 4 °C . After, 95 μL of supernatant containing the MVs were resuspended in 400 L of 1x binding buffer and incubated in the dark for 30 min at room temperature, with 5 L of annexin V . MVs-annexin V-positive were quantified by flow cytometry. The assessment of fluorescence was performed with FACSCantoTM II, BD Biosciences, San Jose, CA, USA. For each sample, 20,000 events were recorded.
Digital holographic microscopy
The impact of HgCl2 on RBC morphology was assessed using a Digital Holographic Microscopy (DHM® T1000 microscope) (Lyncée Tec SA, Lausanne, Switzerland) equipped with a motorized microscope stage (Märzhäuser Wetzlar GmbH & CO. KG, Wetzlar, Germany), an incubator system (LCI Live Cell Instrument, Seoul, South Korea), and a 20×/0.40 NA objective (Leica Microsystems GmbH, Wetzlar, Germany), as described in Bardyn et al. [30, 36]. DHM is a label free microscopy using a low intensive laser source limiting cell alteration. This technique is based on the quantitative measurement of the optical pathlength (OPL) delay (interferometric phase shift measurements) induced by the sample . This parameter is linked to the cell volume and refractive index. The DHM images were analyzed with the software CellProfiler (Analyst) that classes the RBC in predefined morphological categories and then quantifies the different morphological types [38, 39].
As before, RBC were suspended to 10 % hematocrit and treated with HgCl2 (10, 20 and 40 µM). Subsequently, RBC were diluted in Krebs solution and 100 µL, containing 80,000 RBCs, were seeded per well, as quadruplicates, in a 96-well black imaging plate coated with poly-L-ornithine . To accelerate cell sedimentation, the plate was centrifuged (140 g for 2 min at RT).
For imaging, the plate was put under the microscope in the incubation chamber set at 37 °C and 5 % CO2. Four images were taken per well at 20× magnification.
Data evaluations were expressed as means ± S.D. of three independent experiments performed in triplicate with RBC from six donors. The significance of differences was determined by one-way and two-way ANOVA followed by a Tukey’s and Dunnet’s multiple comparisons test. GraphPad Prism 9.1 was utilized for statistical analyses.
Electrophoretic analyses of membrane proteins and Western blotting of Ankyrin and Flotillin-2 from Hg-exposed RBC
In order to explore the possible interaction of Hg with RBC membrane proteins, intact human RBC were exposed in vitro for 24 h in the presence of increasing HgCl2 concentrations (10-40 μM) and the electrophoretic profiles of the membrane fraction were evaluated. The typical SDS-PAGE electrophoretic profile of RBC membrane proteins is shown in Fig. 1. Exposure of cells to all tested HgCl2 concentrations resulted in a significant alteration in the electrophoretic profile. Therefore, with the aim of clearly identify the specific Hg-modified RBC membrane proteins, the effect of Hg on Ankyrin and Flotillin-2, proteins essential for the membrane integrity, was quantified by Western blot.
Fig. 2 and 3 show that both proteins of interest, Ankyrin and Flotillin-2, were detected at their molecular weights (190 and 47 kDa, respectively). Their amounts significantly increased after overnight Hg-treatment (range 10-40 μM) in contrast to those in untreated cells (CTR). In particular, Ankyrin showed an increase in a dose-dependent manner, with a significant effect starting at concentrations as low as 10 μM and reached a plateau after 20 μM. As for Flotillin-2, the addition of HgCl2 10 μM had no effect whereas fold-changes of 2 and 4 were observed for 20 and 40 μM, respectively.
Effect of mercury on sulphate uptake in RBC
B3p-Ankyrin binding appears to be crucial for the proper functioning of both proteins. Consequently, the effect of Hg on the ionic transport function of B3p was analyzed. The efficiency of B3p can be monitored by determining the rate constant for SO42- uptake, which is slower and more easily detectable than Cl- or HCO3 - uptake. SO42- uptake kinetics (as a measure of the level of anion transport) in RBC treated with different concentrations of HgCl2 (10, 20 and 40 μM) or with the B3p inhibitor DIDS (10 μM) are shown in Fig. 4. All treatments significantly reduced the uptake rate of SO42- compared with controls. In addition, RBC treated with DIDS showed similar degrees of saturation. It clearly indicates that Hg inhibited the B3p transport function.
Effect of Hg on PS-bearing MVs release from RBC
PS externalization on MVs were identified based on binding to annexin-V. It is known that increased MVs exposing PS are involved in prothrombotic effects [40–42].
As illustrated in Fig. 5, differences in PS exposure on MVs membrane were observed. In particular, we observed a dose-dependent exposure, consequently, Hg at higher concentrations also supports PS exposure in MVs.
Effect of mercury on RBC morphology
Cell morphology was observed using DHM imaging. Fig. 6 shows the effect of HgCl2 on RBC morphology after 24 hours of incubation at 37 °C. The proportion of different morphological RBC types with respect to the total RBC populations presented in Fig. 6 (A). Seven RBC shape types were identified (see Fig. 6B) and classified as follows: discocytes, corresponding to the physiological shape; stomatocytes, echinocytes I, II and III (intermediate transition between discocytes and spherocytes characterised by the presence of a respectively increasing number of spicules), and the last stage of RBC aging sphero-echinocytes and spherocytes.
As a global trend after 24 h of incubation, the addition of HgCl2 induced decreases of discocytes from 35 (CTR) to 24% (HgCl2 40 μM) and echinocytes (I) from 42 to 16.5% and concomitant increases of echinocytes (III) from 0.9 to 7.1%, sphero-echinocytes from 1 to 8.9% and spherocytes from 1.7 to 16%; as for the echinocytes (II) no difference was observed between all conditions. It highlights a clear shift from reversible to irreversible morphologies. Moreover, the 10 μM had a moderate effect, whereas the addition of 40 μM of HgCl2 significantly affected the RBC.
R.N. (methodology; investigation; visualization; review and editing). E.L. (writing—original draft preparation; review and editing; data curation). P.P. (software; investigation; writing—original draft preparation). D.C. (software; formal analysis). M.P. (validation; writing—review and editing; supervision; visualization). C.M. (Conceptualization; validation; writing—review and editing; supervision).
E.L. received financial supports from The SRTS VD foundation.
Statement of Ethics
Informed consent was obtained from all subjects involved in the study.
The authors have no conflicts of interest to declare.
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