The Gardos channel is a Ca2+ sensitive, K+ selective channel present in several tissues including RBCs, where it is involved in cell volume regulation. Recently, mutations at two different aminoacid residues in KCNN4 have been reported in patients with hereditary xerocytosis. We identified by whole exome sequencing a new family with two members affected by chronic hemolytic anemia carrying mutation R352H in the KCNN4 gene. No additional mutations in genes encoding for RBCs cytoskeletal, membrane or channel proteins were detected. We performed functional studies on patients’ RBCs to evaluate the effects of R352H mutation on the cellular properties and eventually on the clinical phenotype. Gardos channel hyperactivation was demonstrated in circulating erythrocytes and erythroblasts differentiated ex-vivo from peripheral CD34+ cells. Pathological alterations in the function of multiple ion transport systems were observed, suggesting the presence of compensatory effects ultimately preventing cellular dehydration in patient’s RBCs; moreover, flow cytometry and confocal fluorescence live-cell imaging showed Ca2+ overload in the RBCs of both patients and hypersensitivity of Ca2+ uptake by RBCs to swelling. Altogether these findings suggest that the ‘Gardos channelopathy’ is a complex pathology, to some extent different from the common hereditary xerocytosis.
The Gardos channel is a Ca2+ sensitive, intermediate conductance, K+ selective channel present in several cell types including red blood cells (RBCs)1, where it is involved in cell volume regulation. Activation of the channel in response to elevation of cytosolic Ca2+ in human erythrocytes causes transient cell shrinkage due to the efflux of K+ and concomitantly of Cl−, a phenomenon referred to as Gardos effect2. Patch-clamp experiments have shown that local membrane deformations may act as a stimulating event leading to Gardos channel activation in RBCs, providing evidence for the role of this mechanosensory mechanism in shaping and volume modifications of erythrocytes3.
In the last years Gardos channel has been identified as an interesting therapeutic target in human diseases4, 5; in particular, its inhibition in sickle cell disease patients has shown to reduce RBC dehydration and hemolysis, and to increase hemoglobin levels despite the lack of any reduction in the frequency of pain episodes6,7,8.
Gardos channel (KCa3.1) is a tetramer of 4 identical subunits, encoded by the KCNN4 gene9. Recurrent mutations at two different aminoacid residues in KCNN4 (R352H, V282M/E) have been reported in patients from 6 independent families with dehydrated hereditary stomatocytosis (DHSt)10, 11, 12. In a recent paper aimed at studying the effect of the Gardos channel inhibitor Senicapoc, it was observed that the three mutants result in a higher channel activity, although they do not share a common mechanism in altering channel characteristics, i.e. Ca2+ sensitivity13. However, the link of the Gardos channel dysfunction to increased hemolysis has so far not been elucidated.
To get a mechanistic link between the Gardos channel mutation, the cellular properties and eventually the clinical phenotype, we studied two novel patients carrying KCNN4 R352H mutation performing the following investigations: (a) single cell patch-clamp recordings on both RBCs and RBCs precursors, (b) measure of the activity of single ion transporters using 86Rb+ as a tracer for K+ flux experiments, (c) evaluation of intracellular ions contents and RBC glycolysis (d) Ca2+ handling by fluorescence live imaging and flow cytometry on RBCs. We found pathological alterations in the functions of multiple ion transport systems, and metabolic glycolytic impairment.
The proband (II.4), a 40 years old man of Northern Italian origin, was referred to our Centre for the first time at the age of 3 months for evaluation of hemolytic anemia and hepatosplenomegaly; the unrelated parents and three siblings were hematologically normal. Hb levels ranged 7–9 g/dL, reticulocytes 250–350 × 109/L, osmotic fragility was decreased or normal, no defects of RBC enzymes were detected. Bone marrow (BM) analysis revealed erythroid hyperplasia, and measurement of RBC survival showed reduced lifespan with intra-splenic hemolysis. The patient was occasionally transfused during spontaneous hemolytic crises; at the age of 11 he underwent splenectomy and cholecystectomy at 13. After splenectomy Hb levels were maintained around 10 g/dL, no further transfusions were required, thromboembolic events never occurred. Fibroscan, Magnetic Iron Detector (MID) and liver iron concentration showed moderate iron overload, consequently iron chelation was started.
Proband’s first daughter (III.1), born at term after an uneventful pregnancy, presented severe anemia requiring RBC transfusion at birth (Hb 6.1 g/dL) and at 3 months. Afterwards, until the age of 2 years, Hb levels stabilized to about 10 g/dL with no need of further transfusions. Her mother was hematologically normal.
Clinical and hematologic data at the time of the study are reported in Table 1. Both patients displayed moderate hemolytic anemia, reticulocytosis and abnormal RBC morphology with marked anisopoikilocytosis and stomatocytosis. BM examination in II.4 revealed erythroid hyperplasia with some dyserythropoietic changes, in particular binucleated erythroblasts (Supplementary Figure 1).
The osmotic gradient ektacytometry did not display the leftward shift of the curve typical of DHSt in both patients (Omin 142 and 149 respectively for II.4 and III.1, n.v. 136–152; OHyper 457 and 437, n.v. 446–474) (Fig. 1A), in spite of the presence of stomatocytes in the peripheral blood smear. No differences were observed by performing Osmoscan curve in different conditions (fresh blood, 24 h incubation at 4 °C) and with different anticoagulants (heparin, EDTA).
The RBCs filterability was decreased in patient II.4 (splenectomized) and normal in III.1 (not splenectomized, infant). To verify that cells needed to deform in this procedure, we compared untreated healthy cell with cells where mechano-sensitive channels were inhibited by preincubation with 5 µM GsMTx-4. To assess the contribution of the Gardos channel in filterability we pretreated cells with 10 µM of the Gardos-channel inhibitor TRAM-34. Both treatments resulted in a significant decrease in filterability compared to untreated controls. Pre incubation with 5 µM GsMTx-4 and TRAM-34 together caused further decrease in filterability (Fig. 1B).
Percoll density gradient separation showed an increased high-density cell fraction in both patients; medium-density fraction was shifted somewhat upwards in patient II.4 indicating an increase in MCV and a decrease in the average RBC density (Fig. 1C). Plasma of patients’ blood samples contained free hemoglobin. Hemolysis was most pronounced in II.4 sample showing disturbed filterability.
Taken together, the above reported results, in particular Osmoscan and filterability data, indicate that despite presence of stomatocytes, patients’ RBC didn’t show the expected dehydration. The slight differences in RBCs properties observed between III.1 and II.4 could be attributed to infant/adult age of the two patients and presence/absence of the spleen.
All the family members underwent whole exome sequencing. Only one candidate gene (KCNN4) was identified by non-synonymous heterozygous mutations with expression in hematopoietic tissues. A de novo heterozygous missense mutation (c.1055G > A, p.R352H) was detected in II.4 and dominantly transmitted to the daughter III.1 (Fig. 2A). The mutation falling in exon 7 is involved in the calmodulin binding domain (CaMBD) (Fig. 2B). The mutation was confirmed by Sanger sequencing. No additional mutations in genes encoding for RBCs cytoskeletal, membrane or channel proteins were detected by whole exome sequencing in the affected patients.
Functionality of the mutated Gardos channel
Gardos channel activity was evaluated measuring whole-cell currents by patch-clamp and K+(86Rb+) influx from mature RBCs.
Figure 3A–C summarizes the whole-cell measurements showing raw current traces (Fig. 3A), I-V-curves (Fig. 3B), a comparison of the percent block by 1 μM TRAM-34 of the current at −110 mV (control vs. patient II.4, Fig. 3Ca) and an assessment of the difference (with and without 1 μM TRAM-34) in the standard deviation (SD) of the current at −110 mV (control vs. patient II.4, Fig. 3Cb). Application of the Gardos channel blocker TRAM-34 reduces current amplitudes in RBCs of both healthy controls and patient II.4 (Fig. 3B). The effect of TRAM-34 is mostly pronounced at very negative voltages; this is fully compatible with the considerable inward rectification reported for the channel14 and was similarly detected in the comparison between RBCs of KCa3.1-knock-out and wild type mice15.
As shown in Fig. 3Ca, the patient’s cells show a tendency for an increased percentage of current block by TRAM-34 as assessed by mean-currents, although not statistically significant (p = 0.08); the patient’s channel activity is clearly increased as judged by the comparison of the difference in the SD of current with and without TRAM-34, such a difference being a read-out for Gardos currents even in cells expressing a few channels (Fig. 3C). In the whole-cell configuration the cytosolic Ca2+ is equilibrated with the pipette solution, i.e. equal Ca2+-concentration for patient II.4 and healthy controls.
These data confirm that KCNN4 R352H mutation is a gain-of-function mutation leading to increased channel activity.
Differences in current properties are not only characteristic of the circulating cells, but can also be tracked down to the polychromatic erythroblasts (EPCs) differentiated for 11–13 days ex vivo from the peripheral CD34+ cells. We detected an abnormal voltage-sensitivity of the Ca2+ and TRAM-34 sensitive current component in EPCs of the II.4 patient. Whereas erythroblasts produced from the CD34+ cells derived from healthy donors were insensitive to multiple depolarization-repolarization cycles, EPCs of patient II.4 responded to a repeated voltage steps protocol with a progressive increase in current within the positive potential range (Fig. 4). This increase in channel activity was associated with cell swelling that could be observed microscopically during the voltage-clamp recordings (data not shown). The depolarization-inducible current could be blocked by omission of Ca2+ from the extracellular solution, TRAM-34 supplementation, or addition of methyl isobutyl amiloride (MIA), an inhibitor of the Na+/H+-exchanger that prevented swelling in response to the ramp protocol application. These findings suggest an existence of a cross-talk between the Na+ uptake and swelling induced by the repeated changes in the transmembrane potential on one hand, and K+ loss through the Gardos channels on the other.
We further extended our studies of ion movements through the RBC membrane to monitoring the unidirectional K+(86Rb+) influx in cells of II.4. The fraction of K+ uptake through the Gardos channel was detected as the flux sensitive to TRAM-34. This component was small, but detectable in RBCs of the II.4 patient, whereas it was below detection limits in the cells of the healthy donor (Fig. 5A).
Activity of electroneutral transporters, Na,K-ATPase and glycolysis in mature RBCs
Hyper-activation of K+ flux through the Gardos channel in patient’s RBCs was accompanied by abnormally high activity of chloride-dependent K+ flux mediated by Na,K,2Cl- and K,Cl-cotransporters. Abnormally high passive K+ loss was compensated by a 4-fold increase in Na,K-ATPase activity in patient’s RBCs (Fig. 5A). Intracellular Na+ content in RBCs of II.4 was doubled when compared to the healthy control (Fig. 5B), despite the dramatic increase in the active Na+ extrusion by the Na,K-ATPase. Ion gradients in II.4 were maintained at a cost of ATP reduction (Fig. 5C), and stimulation of glycolysis in RBCs (could be observed as a facilitated depletion of plasma glucose and faster lactate production during 24 h of storage at room temperature (Glucose 2.45 vs. 3.20 mM and Lactate 8.25 vs. 5.6 mM in II.4 and control, respectively).
Calcium handling in patients with mutated Gardos channel
We measured intracellular Ca2+ levels in RBCs of II.4, III.1 and controls using fluorescence live imaging and flow cytometry. Figure 6A depicts the representative confocal images of fluo-4 fluorescence intensity proportional to the amount of free Ca2+. We observed an increased heterogeneity in the Ca2+ content and higher number of RBCs with extraordinary high free Ca2+ levels and eventual sequestration of Ca2+ in intracellular vesicles. Figure 6B shows statistical analysis of Ca2+ contents. The abnormally high and heterogeneous intracellular Ca2+ content was also confirmed by flow cytometry in both patients. The absence of splenic sequestration of more compromised cells in patient II.4 may justify the higher Ca2+ content respect to III.1. The observation of high intracellular Ca2+ hints to an increased activity of Ca2+-permeable ion channels such as PIEZO-1, the transient receptor potential cation channels (TRPC6), the voltage-dependent anion selective channels (VDACs), or N-methyl aspartate receptors (NMDARs), suggesting that mechanical stimulation could be involved in tuning the activity of multiple ion transport pathways.
We therefore tested the sensitivity of Ca2+ uptake to mechanical stimulation (swelling). Hypoosmotic swelling was induced by acute supplementation of water to decrease the osmolarity to 220 mOsm. Intracellular Ca2+ was measured before and immediately after reduction of the osmolarity. As shown in Fig. 6(C–F), swelling triggered massive Ca2+ uptake in RBCs of both patients and controls. Intracellular free Ca2+ levels reached in the swollen cells of III.1 and, in particular, of II.4 substantially exceeded those measured in the RBCs of healthy subjects revealing abnormally high Ca2+ uptake in both patients.
These observations were in line with the sensitivity of the abnormally high ion currents in the EPCs of II.4 patient, not only to TRAM-34 and omission of Ca2+, but also to MIA that abolished swelling of EPCs in response to the repetitive ramp protocol application (Fig. 4B).
In this paper we report a new family with two members affected by chronic hemolytic anemia associated with the R352H mutation in the KCNN4 gene encoding the Gardos channel.
Mutation R352H is located in the calmodulin binding domain of the Gardos channel. As also shown by Rapetti-Mauss et al.10, 13, the mutation not only changes the Ca2+ sensitivity affecting the channel threshold of activation, but modifies its functional properties per se resulting in a more active channel, the higher activity possibly due to altered open probability or unitary conductance.
The slightly bigger endogenous current observed in the case studied by Rapetti-Mauss et al.13, compared to our observations may be explained by differences in measurement protocols or sample handling, such as applying voltage ramps compared to discrete voltage steps, associated differences in the holding potential or RBC storage before performing the recordings16.
In this study we also show that differences in current properties are not only characteristic of the circulating RBCs, but can also be tracked down to erythroblasts differentiated ex vivo from peripheral patient CD34+ cells. The effects in precursor cells are more pronounced compared to mature circulating RBCs (Fig. 4 vs. Fig. 3), which is not surprising regarding the low abundance of the Gardos channel in mature circulating RBCs. Based on patch-clamp recordings Grygorczyk et al.14 estimated that approximately 75% of RBCs have between 1 and 5 channels per cell whereas the rest have approximately 11 to 55 channels per cell; Wolff et al.17 estimated an even lower number of an uniform mean of 1 to 3 channels per cell.
To get a mechanistic link between the Gardos channel R352H mutation, the cellular properties and eventually the clinical phenotype, we also measured the activity of single ion transporters using 86Rb+ as a tracer for K+ flux experiments, we evaluated the intracellular ions contents and the effects on RBC glycolysis. The observation of a 3–4 fold increase of unidirectional K+(86Rb+) fluxes in patient II.4 suggests that mutant R352H activate a series of compensatory processes resulting in the prevention of terminal dehydration.
A possible scenario is presented in the scheme reported in Fig. 7. Following the increased activity of the mutated Gardos channel and the subsequent excessive loss of cell K+, K+ influx through NKCC and possibly KCC, is enhanced. Moreover, the NKCC-mediated Na+ accumulation is further enhanced by activation of the Na+/H+ exchanger (NHE) as confirmed by our patch-clamp data on erythroid cells using NHE specific inhibitors and in line with the increase of the intracellular Na+ content observed in the splenectomized II.4 patient. The abnormally high intracellular Na+ content results in cell swelling, triggers activation of the Na,K-ATPase and increases energy consumption18, 19 as demonstrated by the ATP reduction and stimulation of glycolysis. Interestingly we found Ca2+ overload and increased heterogeneity of the inter- and intra-cellular distribution of Ca2+ in RBCs of both patients as assessed by flow cytometry and confocal fluorescence live-cell imaging. Such an overload could possibly be aided by activation of the mechanosensitive, thus swelling activated, PIEZO1 channels or through other Ca2+ entry pathways e.g. voltage-sensitive cation channels; these latter are possibly implied as observed by the increase of EPCs current as a result of repeated voltage ramps, then abolished by external Ca2+ removal.
Increase of the Ca2+ content in patients RBCs may trigger numerous Ca2+-dependent processes20 such as scramblase activation, calpain cleavage, flippase inhibition and ultimately provides a positive feedback loop for the Gardos channel itself. The markedly up-regulated intracellular Ca2+ levels in RBCs may contribute to premature removal of these RBCs from the circulation21. Thus based on our data, a point mutation in a single channel present in a low number of copies (3–200/cell according to different authors)14, 17, 22 in RBCs may interfere with the regulation of multiple ion transport systems and, consequently, with metabolic rates, membrane stability and cellular morphology of circulating RBCs as well as erythroblasts.
Recently, in a very short period of time, three different groups described mutations in the KCNN4 gene associated with DHSt10, 11, 12; our report brings to 7 the number of affected families. The identification of R352H as a de novo event in patient II.4 reinforces the hypothesis that it could be a mutational hotspot11.
The patients with KCNN4 mutations reported so far display a wide phenotypic heterogeneity, ranging from severe fetal anemia requiring in utero transfusions to mild or compensated hemolysis (Supplementary Table I). It is worth mentioning that all the 8 splenectomised patients do not display the increased susceptibility to thrombotic events commonly reported in DHSt23, 24; this holds especially true when considering the very long follow-up after splenectomy of patient II.4. An explanation for such an observation may reside in the increasingly recognized interplay between mechano-sensitive channels like PIEZO1 and the Gardos channel3, 25. When passing capillaries or other constrictions of smaller diameter, the RBCs mechano-sensitive channels that conduct Ca2+ are activated and the consecutive Ca2+-flashes activate Gardos channels for a fast and transient volume adaptation. This concept is supported by our measurements of filterability, since both inhibition of mechano-sensitive channels (with GsMTx-4) and inhibition of the Gardos channel (with TRAM-34) decrease filterability. Thus if the function of mechano-sensitive channels is impaired, such as Piezo1 in typical DHSt26, the above described volume adaptation does not work properly, RBCs can get stuck and form aggregates caused by intercellular adhesion27. In the presence of the spleen, RBCs lacking the adaptive volume regulation get stacked in the splenic slits and are consecutively removed, whereas in splenectomized patients they circulate leading to thrombotic events. In patients with the KCNN4 mutation, Gardos channels are more sensitive to Ca2+ and more active, and with such compensation at hand, volume adaptation is less impaired suggesting a reduced post-splenectomy thrombotic risk, to be confirmed in further studies.
The dyserythropoietic features detected in the bone marrow of II.4 supports the hypothesis that KCNN4 may play a role in erythroid maturation, suggested also by the I-V-curves in precursor cells indicating a higher abundance of Gardos channels in erythroid precursors compared to mature RBCs; therefore, iron overload detected in our and other patients with KCNN4 mutation11 may be a consequence of dyserythropoiesis, similar to what is reported in DHSt with PIEZO1 mutations28, 29. The history of the patients reported here confirms that congenital hemolytic anemia due to abnormal cation permeability may represent a diagnostic challenge that is now overcome by means of the new Next Generation Sequencing technology approaches. Patient II.4 received a diagnosis of hereditary spherocytosis in infancy and was splenectomized without clinical improvement; the finding with SDS-PAGE of a spectrin deficiency may be considered a secondary effect of a membrane perturbation30, 31 disclosed by splenectomy32, since it is absent in the daughter, and no mutations in the spectrin or other related genes were detected by whole exome sequencing. The phenotypic variability, the possible high frequency of de novo variants, and the absence of specific biological tests make the diagnosis of this variant of hereditary stomatocytosis particularly difficult. The widespread use of NGS technology is likely to result in a greater than expected frequency of Gardos channelopathies.
In conclusion, this study shows that KCNN4 R352H mutation determines, together with an increased Gardos channel activity, an unexpected activation of multiple compensatory changes, in absence of any other abnormalities of red cell membrane or channel proteins.
We suggest that the ‘Gardos channelopathy’ is a more complex pathology, to some extent different from the common DHSt type, and that distinct mutations in the Gardos channel may have a diverse impact on cell volume regulation mechanisms. In fact, as shown in Supplementary Table I, patients with R352H mutation are characterized by milder dehydratation and normal Osmoscan curve when compared to V282M/E cases that display typical features of hereditary xerocytosis33, 34, (median MCHC R352H 35 g/dL vs. MCHC V282M/E 36.4).
This observation is also in line with the recent study by Rapetti-Mauss et al. aimed to define the sensitivity of KCNN4 mutants to Senicapoc, where it was demonstrated that the three mutations (R352H, V282M/E) do not share a common mechanism in altering channel characteristics and display significantly different Senicapoc sensitivity13, 35. Further investigation of the molecular mechanisms behind the cross-talk between numerous ion transporters and exploration of the causes of the abnormal hyper-sensitivity to mechanic stimulation and of Ca2+ overload may give more clues to the optimization of diagnosis and therapeutic approaches for this group of patients.
All the diagnostic procedures and investigations were performed in accordance with the Helsinki Declaration of 1975. Patients had given their consent for the participation to this study. The study was approved by Ethical Committee at Fondazione IRCCS Ca’ Granda Ospedale Maggiore of Milan.
Routine hematological investigations were carried out according to Dacie & Lewis36. RBC osmotic fragility was evaluated by NaCl test on fresh and incubated blood at 37 °C overnight, acidified glycerol lysis test (AGLT), and Pink test as described elsewhere37. EMA-binding was performed by the method of King et al.38, RBC enzymes’ activities were determined according to Beutler39, and membrane proteins were analyzed by SDS-PAGE40, 41.
Osmoscan was performed by Laser-assisted Optical Rotation Cell Analyzer (LoRRca MaxSis, Mechatronics, Hoorn, The Netherlands) following the manufacturer’s instructions; samples were tested in different experimental conditions (fresh blood, after 24 h at 4 °C) and drawn in Heparin and EDTA to ascertain whether incubation and anticoagulants may affect the curve as hypothesized by Badens & Guizouarn42. The Osmoscan curve performed after 24 h incubation at 37 °C was markedly altered in both patients and controls.
All the analyses were performed with cells of patient II.4, and of patient III.1 when feasible due to the limitation of blood sample size (child).
Next Generation Sequencing
Library preparation, Whole Exome Sequencing and data analysis, performed before the report in literature of new mutations in KCNN4, were provided as service by Genomnia srl (Lainate, Italy), using the Life Technolgies SOLiD 5500xl Genetic Analysis Sequencer. For details please refer to Supplementary Information.
The mutation was confirmed by Sanger sequencing (ABI PRISM 310 Genetic Analyzer, Applied Biosystems).
Isolation and culturing of erythroid precursor cells (EPCs)
Heparinised peripheral blood (PB) samples of patient II.4 and a healthy control were obtained and processed within 5 h after collection. Mononuclear cells were isolated on a Ficoll-Paque PLUS gradient (GE-Healthcare, Dietikon, Switzerland), and cultured in a two-phase liquid system as described elsewhere43. Late-stage erythroblasts were then used for assessment of electric currents across the EPCs membranes by means of patch-clamp.
The filterability test was performed with RBCs of patients II.4 and III.1 and controls by a modified method originally developed by Beutler et al.44 for the depletion of leukocytes. To assess the impact of mechano-sensitve channels and Gardos channel into filterability, healthy RBCs were treated with the blocker of mechano-sensitive channels (GsMTx-4) and the Gardos channel blocker TRAM-34 prior to the filtration onset. For a detailed description please refer to Supplementary Information.
Separation of RBCs on Percoll density gradient
Separation of RBCs into the low (L), medium (M) and high (D) density fractions was performed as described elsewhere . Whole blood (1–1.5 mL) was overlayed on 12.5 mL 90% isotonic Percoll solution (GE Healthcare; density 1.130 g/mL) prepared by mixing 90 mL of Percoll with 10 mL × 10 PBS (Sigma-Aldrich) and 11 mL × 1 PBS (Sigma-Aldrich). The resulting samples were centrifuged using Sorvall RC-5C plus centrifuge equipped with a SM-24 rotor at 4 °C for 30 min at 45,000× g.
Patch-clamp measurements on circulating RBCs were performed with a NPC-16 Patchliner (Nanion Technologies, Munich, Germany) and on the EPCs of patient II.4 with a conventional patch-clamp setup (Axon CNS, Molecular Devices, Downingtown, PA, USA) The resistance of the chips with internal and external solutions as follows (in mM): KCl 70, KF 70, HEPES 30, CaCl2 0.5, pH = 7.2 adjusted with KOH (internal) and KCl 140, MgCl2 5, CaCl2 6, D-glucose 2.5, HEPES 10, pH = 7.3 adjusted with KOH (external) was between 5 and 8 MΩ. Gigaseals were considered successful if exceeding 5 GΩ (with most cells they were 10 GΩ and above). Gigaseal formation was facilitated by the use of a seal enhancing solution as recommended by the Patchliner manufacturer and containing (in mM): NaCl 80, KCl 3, MgCl2 10, CaCl2 35, HEPES 10, pH = 7.3 adjusted with NaOH. The seal enhancing solution was only used to help obtaining the very high gigaohmic contact between the cell and the chip and in the whole-cell configuration was replaced by the external solution. Whole-cell configuration was achieved by negative pressure suction pulses between −45 mbar and −150 mbar and its formation judged by the appearance of sharp capacitive transients. Whole-cell patch-clamp recordings were conducted at room temperature using voltage steps from −130 mV to 70 mV for 500 ms in 20 mV increments at 5 s intervals, the holding potential being set at −30 mV. Gardos current differences between patient II.4 and healthy donors were assessed by comparing the block of currents by 1 µM TRAM-34. To reduce inter-cell variability data are expressed as normalized current which is the ratio of the current under specified experimental conditions i.e. before (control) and in the presence of 1 µM TRAM-34 at selected membrane potentials, to the current at +70 mV determined 30–60 s before starting the control (control) measurement. Data are presented as means ± SEMs (n represents the number of cells).
Such an approach to avoid inter-cell variability we have successfully used45. A two-tailed, paired t-test was applied on the normalized currents to assess the difference in the current with and without 1 µM TRAM at every potential.
Assessment of the fluctuations of the current (obvious in Fig. 3A Ctrl-basal and II.4-basal and abolished by TRAM as seen in Ctrl-TRAM and II.4-TRAM) allowed us to account also for the cells with only a few channels. Analysis of the kinetics of the traces giving us a sensitive quantitative measure of the Gardos channel activity in all cells was done in the following way: we considered the variance of the current trace at −110 mV for each cell. From the variance we calculated the standard deviation for the trace (this was done separately for the trace without TRAM and for the trace with 1 μM TRAM). We then subtracted the two standard deviations (these are paired data of the same cell). This difference was considered as a read-out of the Gardos channel activity (more fluctuations = higher activity). 23 cells from the patient and 27 cells from the control were compared using a non-paired t-test (Fig. 3Cb).
Electric currents through the membranes of EPCs of a patient (II.4) were assessed as described elsewhere46. Whole-cell voltage clamp experiments were performed during ex-vivo hematopoiesis between day 11 and day 13. EPCs were plated on poly-L-lysine (0.01% vol/wt in H2O) coated cover glass slides and voltage-clamped at room temperature under constant perfusion with extracellular solution. For data acquisition and analysis the Axopatch 200B amplifier, Digidata 1440A, and pClamp 10.3 were used (all by Axon CNS, Molecular Devices, Downingtown, PA, USA).
The leak current was subtracted manually and the data were filtered at 5 kHz. A voltage-step protocol was used to asses the passive electrophysiological properties. The voltage was hold at −70 mV and stepped for 200 ms from −120 mV to +80 mV, in 10 mV increment. The protocol was repeated 1–3 times. The standard intracellular solution consisted of (in mM) 117 KCl, 11 HEPES, 1 EGTA, 10 NaCl, 2 MgCl2, 2 Na2ATP, adjusted to pH 7.2 with KOH was used. The standard extracellular solution consisted of (in mM) 135 NaCl, 5 KCl, 5 HEPES, 10 D-glucose, 1.5 CaCl2, adjusted to pH 7.35 with NaOH. When stated, extracellular solution was Ca2+-free and containing 1 mM EGTA or supplemented with the inhibitor of the Na+/H+ exchanger methyl isobuthyl amiloride (MIA) and blocker of Gardos channel TRAM-34 (final concentration for both blockers was 15 µM). To ensure fast drug application, a Rapid Solution Changer System was used, which allowed solution changes within 20 ms. Data are presented as means ± SEM.
K+ (86Rb+) influx
Unidirectional influx rates for K+ were assessed by using 86Rb+ as a tracer as previously described47. Total unidirectional K+ influx was detected in erythrocytes incubated at hematocrit of 5–8% in the standard incubation medium containing (in mM): 145 NaCl, 4 KCl, 0.15 MgSO4, 2 CaCl2, 10 glucose, 10 sucrose, and 10 HEPES-Tris, 0.3 L-arginine, 0.3 L-glutamate, and 0.3 L-glycine, pH 7.4 at 37 °C. Chloride-free medium contained (in mM): 145 NaNO3 and 4 KNO3 instead of NaCl and KCl respectively. Ouabain (final concentration 100 µM), and TRAM-34 (10 µM) were used as selective blockers of the Na,K-ATPase, and the Gardos channel, respectively. Cells were pre-incubated for 15 min to enable binding of the inhibitors to their targets. Influx was then initiated and measured by addition of 86RbCl (104 Bq/mL) and aliquots of the RBC suspension collected 10, 20, 30, 45, and 60 min after the onset of incubation. The cells were washed free from extracellular tracer, lysed and the amount of 86Rb+ accumulated in erythrocytes was measured and normalized to the amount of the radioactive tracer in the incubation medium. Ouabain-sensitive K+ influx was denoted as active K+ uptake by the Na,K-ATPase. Chloride-dependent K+ influx in the presence of ouabain represented cumulative activity of the Na-K-2Cl- and K-Cl-cotransporters. Treatment with TRAM-34 in the presence of ouabain resulted in the inhibition of K+ influx through the Gardos channels.
The Ca2+ imaging was performed based on the Ca2+-fluorophor Fluo-4 (Life technologies, Carlsbad, CA, USA) using a set-up as previously described48. Basal Ca2+-related fluorescence was measured as described before49. To evaluate the cellular distribution, confocal images of Fluo-4 loaded RBCs were recorded on a TCS SP5 (Leica, Mannheim, Germany)50.
Detection of the intracellular Ca2+ levels in RBCs by flow cytometry
Intracellular Ca2+ levels in RBC fractions of healthy control subjects as well as of II-4 and III-1 patients were detected by flow cytometry. 2 µL of whole blood suspended in the incubation medium was loaded Fluo-4 AM (Life technologies, Carlsbad, CA, USA). Thereafter, Ca2+-dependent fluorescence intensity was measured in RBCs using Gallios flow cytometer (Beckman Coulter). Triple measurements (100.000 cells/measurement) were performed and averaged for each condition.
Due to the RBCs marked heterogeneity in sensitivity to mechanical stimulation, and because Ca2+ uptake is acute and transient, swelling was chosen as the most appropriate approach to study RBCs sensitivity to mechanical stimulation.
Sensitivity of Ca2+ uptake to swelling was tested as follows. Basal intracellular Ca2+ levels in RBCs of patients and controls were measured and then the samples were diluted with distilled water (0.25 mL H2O added to 0.5 mL sample) and Ca2+ measurements repeated directly thereafter.
Unless otherwise stated statistical analysis was performed using one-way ANOVA with Bonferroni’s multiple comparison test or Student’s paired t-test, as appropriate (with normal distribution of the values), Kruskal-Wallis with Dunn’s post test (when the distribution was not normal). For all tests, significance level was set at P < 0.05.
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The authors thank all the members of the family for their contribution to this study; Alessandro Guffanti and Moreno Colaiacovo for fruitful support in NGS data analysis. This study was supported by the Italian Ministry of Health: Ricerca Finalizzata conv n. RF-2010-2303934. The research leading to these results has received funding from the European Seventh Framework Program under grant agreement number 602121 (CoMMiTMenT) and the European Framework “Horizon 2020” under grant agreement number 675115 (RELEVANCE).
The authors declare that they have no competing interests.
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Fermo, E., Bogdanova, A., Petkova-Kirova, P. et al. ‘Gardos Channelopathy’: a variant of hereditary Stomatocytosis with complex molecular regulation. Sci Rep 7, 1744 (2017). https://doi.org/10.1038/s41598-017-01591-w
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