Abstract
Background: Bruton tyrosine kinase inhibitors (BTKi) are used in B-cell malignancies and in development against various autoimmune diseases. Since Btk is also involved in specific pathways of platelet activation, BTKi might be considered to target platelet GPVI/GPIb-mediated atherothrombosis and platelet FcγRIIA-dependent immune disorders. However, BTKi treatment of patients with B-cell malignancies is frequently associated with mild bleeding events caused possibly by off-target inhibition of Tec. Here, we compared the platelet effects of two novel BTKi that exhibit a high (remibrutinib) or low (rilzabrutinib) selectivity for Btk over Tec.
Methods and Results: Remibrutinib and rilzabrutinib were pre-incubated with anticoagulated blood. Platelet aggregation and in vitro bleeding time (closure time) were studied by multiple electrode aggregometry (MEA) and platelet-function analyzer-200 (PFA-200), respectively. Both BTKi inhibited atherosclerotic plaque-stimulated GPVI-mediated platelet aggregation, remibrutinib being more potent (IC50 = 0.03 μM) than rilzabrutinib (IC50 = 0.16 μM). Concentrations of remibrutinib (0.1 μM) and rilzabrutinib (0.5 μM), >80% inhibitory for plaque-induced aggregation, also significantly suppressed (>90%) the Btk-dependent pathways of platelet aggregation upon GPVI, von Willebrand factor/GPIb and FcγRIIA activation stimulated by low collagen concentrations, ristocetin and antibody cross-linking, respectively. Both BTKi did not inhibit aggregation stimulated by ADP, TRAP-6 or arachidonic acid. Remibrutinib (0.1 μM) only slightly prolonged closure time and significantly less than rilzabrutinib (0.5 μM).
Conclusion: Remibrutinib and rilzabrutinib inhibit Btk-dependent pathways of platelet aggregation upon GPVI, VWF/GPIb, and FcγRIIA activation. Remibrutinib being more potent and showing a better profile of inhibition of Btk-dependent platelet activation vs. hemostatic impairment than rilzabrutinib may be considered for further development as an antiplatelet drug.
Introduction
Since the first description of a patient with recurrent infections and deficiency of immunoglobulins termed “Agammaglobulinemia” by Ogden Bruton in 1952 (1), it took more than 40 years of research, until Bruton tyrosine kinase (Btk) was identified in 1993 as the responsible protein that is deficient in patients with X-linked agammaglobulinemia (2, 3). Btk belongs to the Tec (tyrosine kinase expressed in hepatocellular carcinoma) family of non-receptor cytoplasmic tyrosine kinase, and contains five different protein interaction domains: an amino terminal pleckstrin homology (PH) domain, a proline-rich Tec homology (TH) domain, the SRC kinase homology (SH) domains SH2 and SH3, and a kinase domain (4). Btk is the best studied member of this tyrosine kinase family and most homologous to Tec, the namesake of this kinase family. Btk plays a crucial role in B-cell receptor function and in immunoglobulin Fc- receptor signaling of monocytes/macrophages and neutrophils (4). Since the approval of ibrutinib, the covalent irreversible first in class Btk inhibitor (BTKi) in 2013 for treatment of certain B-cell malignancies, many more reversible and irreversible BTKi have evolved and the spectrum of diseases that are targeted extends from specific forms of B-cell malignancies to various autoimmune disorders (5). Up to now four BTKi (ibrutinib, acalabrutinib, zanubrutinib, and tirabrutinib) have been approved but at least further eight BTKi are in clinical studies (5).
Btk is expressed not only in B-cells but also in various hematopoietic cells including the megakaryocyte-platelet lineage (6). Btk in platelets is involved in signaling of specific glycoprotein receptors including glycoprotein (GP) VI activation by collagen, GPIb activation by von Willebrand factor (VWF), FcγRIIa activation by IgG immune complexes, and CLEC-2 activation by podoplanin (5). Thus, Btk might be a promising therapeutic target of platelet-related diseases, and BTKi have indeed been proposed as novel antiplatelet drugs as they inhibit selectively platelet GPVI/GPIb-stimulated atherothrombosis (7, 8), platelet FcγRIIA-dependent immune disorders (heparin-induced thrombocytopenia, vaccine-induced immune thrombotic thrombocytopenia) (9, 10), and podoplanin/CLEC-2 mediated venous thrombosis (11, 12). Somewhat surprisingly, XLA patients do not show a bleeding tendency (13). In contrast, mild bleeding events are frequent in patients with B-cell malignancies treated with irreversible covalent BTKi (ibrutinib, acalabrutinib, zanubrutinib, and tirabrutinib) (5). The reasons are not clear but are probably multifactorial. They might be related to the type of diseases treated, but also caused by off-target inhibition as reviewed recently (5).
Beside Btk the homologous kinase Tec is also expressed in platelets. Whereas, FcγRIIa activation and VWF activation of GPIb do not require Tec activation (5, 9), Tec plays a role in GPVI activation. After GPVI-mediated platelet stimulation by high dose collagen, both Btk and Tec support platelet aggregation. Btk-deficient human platelets from patients with XLA and Btk-deficient mouse platelets do not respond to low concentrations of collagen or collagen-related peptide (CRP) indicating that Btk is required for platelet activation after low-degree GPVI stimulation (14, 15). Similar observations have been made by using low Btk-specific concentrations of irreversible BTKi and the reversible BTKi fenebrutinib which inhibits Btk but not Tec and applying human atherosclerotic plaque which also induces only a low-degree activation of GPVI (8, 9, 16–18). After stimulation with high concentrations of collagen, Tec compensates for the absence of Btk (as in XLA patients) or inhibition of Btk (as after platelet pretreatment with Btk-selective concentrations of BTKi) and preserves GPVI-stimulated platelet aggregation. Inhibition of both Tec and Btk abrogates GPVI-activation (15). Since the four approved irreversible covalent BTKi mentioned above have limited selectivity for Btk over Tec as measured by biochemical assays in vitro (5), and at higher concentrations prolong bleeding time in vitro (19), it is assumed that therapeutic concentrations of these BTKi inhibit in platelets irreversibly Tec in addition to Btk thereby abrogating GPVI signaling. This might contribute to the observed bleeding side effects.
Therefore, we hypothesized that off target effects of BTKi with low Btk selectivity over Tec might explain bleeding of BTKi, and investigated in the present study the effects of two novel BTKi on Btk-mediated pathways of platelet aggregation and bleeding time in vitro: the novel selective covalent BTKi remibrutinib (LOU064), a very potent irreversible covalent BTKi, which is highly selective for Btk and barely inhibits Tec (20), and rilzabrutinib (PRN1008) an oral, reversible covalent BTKi which inhibits Btk and Tec with similar IC50 values (21). Both BTKi are in clinical studies of dermatological autoimmune diseases. Rilzabrutinib inhibits very potently Btk and Tec in vitro (IC50 values, 1.3 and 0.8 nM, respectively) (22). It forms a reversible covalent bond with Cys481 of Btk, and shows a fast association and a very slow dissociation rate (23). Rilzabrutinib is in clinical trials of pemphigus (24) and idiopathic thrombocytopenic purpura (ITP), a disease exhibiting very low platelet counts (<50.000/μl) and bleeding events. Here, it inhibits platelet destruction mainly via the inhibition of autoantibody/FcγR signaling in splenic macrophages (25). Unexpectedly, in a previous report clinically relevant concentrations of rilzabrutinib showed no inhibition of platelet activation in vitro (26).
Materials and Methods
Reagents
Remibrutinib (LOU064), rilzabrutinib (PRN1008) and fenebrutinib (GDC-0853) were purchased from MedChem Express (New Jersey, USA). Dimethyl sulfoxide (DMSO) was from Sigma-Aldrich (Taufkirchen, Germany). Collagen was from Takeda (Linz, Austria). ADP, ristocetin, arachidonic acid (AA) and TRAP-6 (Thrombin Receptor Activator Peptide 6) were obtained from Roche Diagnostics (Mannheim, Germany). The anti-CD32 antibody AT10 (monoclonal mouse IgG1), cross-adsorbed F(ab')2-goat anti-mouse IgG (H + L) and the anti-CD9 antibody Ts9 (monoclonal mouse IgG1) were from ThermoFisher Scientific (Waltham, MA, USA).
Declaration of Helsinki
Informed consent was obtained from healthy volunteers, as approved by the Ethics Committee of the Faculty of Medicine of the University of Munich, and in accordance with the ethical principles for medical research involving human subjects, as set out in the Declaration of Helsinki.
Human Atherosclerotic Plaque Homogenates
Atherosclerotic tissue specimens were obtained from patients who underwent endarterectomy for high-grade carotid artery stenosis. Specimen containing lipid-rich soft plaques were collected. The atheromatous plaques were carefully dissected under sterile conditions from other regions of the atherosclerotic tissue. The plaques were weighed, homogenized with a glass pestle and potter, then stored at −80°C (27, 28). Plaque homogenates from 5 patients were pooled.
Blood Collection
Whole blood from healthy donors who had not taken any antiplatelet drug within 2 weeks was collected by cubital venipuncture into blood tubes (double wall) from Verum Diagnostica GmbH (Munich, Germany) containing hirudin as anticoagulant (final hirudin concentration in blood: 200 U/ml corresponding to 15 μg/ml) for platelet aggregation measurements (29) or buffered trisodium citrate/citric acid solution (citrate concentration 0.129 mol/L; S-Monovette 3.8 mL 9NC/PFA from Sarstedt, Nümbrecht, Germany) for closure time measurements with the PFA-200 (30). The blood was kept at room temperature and measurements were performed with 3 h after venipuncture.
Platelet Aggregation in Blood
Multiple electrode aggregometry (MEA) (Roche Diagnostics, Mannheim, Germany) that monitors the change of conductivity between two sets of electrodes (red and blue traces) caused by the attachment of platelets was applied to measure platelet aggregation, as described (29, 31). In brief, 0.9% NaCl (300 μL) was placed in aggregometer cuvettes (06675590, Roche, Mannheim, Germany) with aliquots (300 μL) of hirudin-anticoagulated blood. BTKi or DMSO (solvent control; 0.6 μL) were added, and mixed well with pipet, covered, and incubated for 1 h at 37°C (19). Then, the cuvettes were transferred into the device, platelet stimuli (collagen, ristocetin, AT10 + Fab2, anti-CD9 antibody, TRAP-6, ADP, or AA) were added at concentrations as detailed in the figure legends, stirring was simultaneously started and aggregation was measured for 10 min. Aggregation was recorded in arbitrary units (AU), and cumulative aggregation (AU*min) from 0 to 10 min was measured by quantifying the area under the curve. The traces selected as representative and displayed in the Figures belonged to a specific experiment whose values were closest to the mean.
IC50 values were obtained by non-linear fitting using the following model:
Fifty = (Top + Baseline)/2
Y = Bottom + (Top-Bottom)/(1 + 10∧((LogAbsoluteIC50-X)*HillSlope + log((Top-Bottom)/(Fifty-Bottom)-1)))
Closure Time Measurement
The INNOVANCE® PFA-200 System (Siemens Healthcare, Erlangen, Germany), which simulates primary hemostasis in vitro, provides rapid and precise assessment of platelet dysfunction and bleeding risk (32, 33). DMSO (0.1%; solvent control) or various concentrations of remibrutinib or rilzabrutinib were pipetted (0.8 μl) into samples of citrate-anticoagulated blood (0.8 ml) (30) and preincubated for 1 h at 37°C. The Dade® PFA Collagen/EPI Test Cartridge was used, and the time of complete plug formation was reported as “closure time.” The normal range of closure time is assessed specifically for each test center and was determined to be 84–170 s. The normal range as recommended by the manufacturer (84–160 s) has been slightly modified at our institution to 84–170 s based on the measurement on 54 healthy unselected persons without any medication according to the approved-level consensus guideline from the Clinical and Laboratory Standards Institute (CLSI EP28).
Statistics
The data are shown as mean ± standard deviation (SD) of the indicated number of the experiments. Normal distribution of values was assessed using the Shapiro-Wilk test. Parallel multi-experimental conditions were analyzed by ordinary one-way ANOVA, followed by Bonferroni's test if the normality test was passed, otherwise a Kruskal-Wallis test for unmatched and a Friedman's test for matched observations followed by Dunn's test were used. Side-by side comparisons were analyzed by Wilcoxon matched-pairs signed rank test.
Results
Remibrutinib (LOU064) and Rilzabrutinib (PRN1008) Dose-Dependently Inhibit GPVI-Mediated Platelet Aggregation in Blood Triggered by Atherosclerotic Plaque
Diverse collagen type I and III fibers are the decisive plaque components that induce platelet aggregation via activation of GPVI (27, 28, 34). Blood was incubated with increasing concentrations of remibrutinib or rilzabrutinib for 1 h prior to plaque stimulation. Remibrutinib and rilzabrutinib inhibited plaque-induced platelet aggregation with IC50 values of 0.03 and 0.16 μM, respectively. Remibrutinib (0.2 μM) and rilzabrutinib (1 μM) were able to block plaque-induced platelet aggregation by >90% (Figures 1A,B). Accordingly, remibrutinib is more potent than rilzabrutinib.
Figure 1
Effects of increasing concentrations of remibrutinib and rilzabrutinib on platelet aggregation in blood stimulated by plaque homogenate. Hirudin anticoagulated blood was preincubated for 1 h at 37°C with solvent control (DMSO, 0.1%), or increasing concentrations of remibrutinib (A,C,D) or rilzabrutinib (B,C,E) and aggregation was recorded for 10 min after stimulation by plaque homogenate (833 μg/ml) (19). The dose-response curves of (A) remibrutinib and (B) rilzabrutinib are shown. (C) Representative aggregation traces in red and blue for each electrode, respectively, are shown. (D,E) Bar graphs show the dose-dependent delay in aggregation by (D) remibrutinib and (E) rilzabrutinib. Single data points are shown but are in part not visible due to overlap. Values are mean ± SD (n = 6). Statistical analysis was carried out comparing against baseline (without BTKi) using the Friedman test followed by Dunn's test (A–E). *p < 0.05, **p < 0.01, ***p < 0.001, ****p < 0.0001.
The aggregation tracings in Figure 1C and panels in Figures 1D,E show a dose-dependent increase in delay of aggregation (lag time) caused by both inhibitors.
Effects of Remibrutinib and Rilzabrutinib on Platelet Aggregation Stimulated by Collagen, Ristocetin, FcγRIIA- and G-Protein Coupled Receptor-Activation
Next the effects of remibrutinib and rilzabrutinib were investigated on platelet aggregation induced by stimuli known to activate Btk-dependent and Btk-independent platelet signaling pathways. Concentrations of remibrutinib (0.1 μM) and rilzabrutinib (0.5 μM) were chosen that inhibited atherosclerotic plaque-induced platelet aggregation by 89 and 88%, respectively (Figure 1A).
Figure 2 shows the results for platelet stimuli that induce aggregation through a Btk-dependent mechanism (5). GPVI-dependent aggregation was inhibited by remibrutinib and rilzabrutinib by 91 and 94%, respectively, on low dose collagen, and by 37 and 41%, respectively, on high dose collagen (Figures 2A,B). Glycoprotein Ib/von Willebrand factor (GPIb/VWF)-dependent ristocetin-induced platelet aggregation was blocked by 95% by both BTKi (Figure 2C). The inhibitory effects of remibrutinib and rilzabrutinib on GPVI- and GPIb/VWF-dependent platelet aggregation were similar to those of fenebrutinib (0.1 μM) (Supplementary Figure 2), which is a reversible and highly selective Btk inhibitor.
Figure 2
Effects of remibrutinib and rilzabrutinib on platelet aggregation in blood after stimulation by collagen, ristocetin or FcγRIIA activation. Hirudin anticoagulated blood was preincubated for 1 h with DMSO or BTKi (remibrutinib 0.1 μM, rilzabrutinib 0.5 μM) prior to stimulation with (A) low dose collagen (0.4–0.6 μg/ml) that was titrated to induce a similar degree of platelet aggregation as plaque homogenate (833 μg/mL) (19), (B) high dose collagen (4–6 μg/ml) that was 10× concentrations of the low dose collagen (8, 19), (C) ristocetin (0.5 mg/ml), (D) CD32 cross-linking (3 min incubation with 2 μg/ml AT10, plus 30 μg/ml Fab2), or (E) anti-CD9 antibody (1 μg/ml). Representative MEA tracings (top panels) and bar graphs (bottom panels) are shown. Values are shown as mean ± SD (n = 5). Statistical analysis was carried out using ordinary one-way ANOVA followed by Bonferroni's test (B,D) or Kruskal-Wallis followed by Dunn's test (A,C,E). *p < 0.05, **p < 0.01, ***p < 0.001, ****p < 0.0001.
Complete suppression of platelet aggregation by both BTKi was also observed on FcγRIIA activation by crosslinking or anti-CD9 antibody stimulation (Figures 2D,E). Due to the absence of adenosine 5'-diphosphate (ADP) secretion from platelets (9), anti-CD9 antibody stimulation showed a delayed aggregation response and less maximal aggregation compared with CD32-crosslinking (Figure 2E).
Remibrutinib and rilzabrutinib did not compromise Btk-independent pathways of platelet aggregation stimulated by GPCR activation with thrombin receptor-activating peptide (TRAP), arachidonic acid (AA), or ADP under the conditions tested (Figure 3).
Figure 3
Effects of remibrutinib and rilzabrutinib on platelet aggregation in blood after stimulation by TRAP, ADP, or AA. Hirudin anticoagulated blood samples were pretreated for 1 h at 37°C with solvent control (DMSO, 0.1%), or BTKi (remibrutinib 0.1 μM, rilzabrutinib 0.5 μM) before stimulation with (A) TRAP (15 μM), (B) ADP (10 μM), or (C) AA (0.6 mM). Representative MEA tracings (top panels) and aligned dot blot bar graphs (bottom panels) are shown. Values shown are mean ± SD (n = 5). Statistical analysis was carried out using ordinary ANOVA followed by Bonferroni's test (A,B) or Kruskal-Wallis test followed by Dunn's test (C), that did not show significant differences.
Effect of Remibrutinib and Rilzabrutinib on in vitro Bleeding Time
To investigate whether remibrutinib and rilzabrutinib might impair primary hemostasis, the platelet function analyzer PFA-200 was used. The instrument aspirates citrate-anticoagulated blood under constant vacuum from a reservoir through a capillary and a small hole in a membrane filter which was coated in our experiments with collagen and epinephrine (collagen/epinephrine cartridge). The time required to obtain full occlusion of the aperture is reported as “in vitro closure time” (32, 35). The PFA is used for routine screening of patients with potential hemorrhagic risk and is very sensitive to monitor aspirin intake (36, 37).
Closure time was slightly, but significantly prolonged by 0.1 μM remibrutinib (Figures 4A,B) which suppressed >85% Btk-dependent platelet aggregation after GPVI activation with low dose collagen and after VWF/GPIb activation with ristocetin (Figures 1A, 2A,C), but it did not exceed the upper limit of the normal range (170 s). Higher concentrations of remibrutinib (0.2 and 0.5 μM) significantly and profoundly prolonged closure time.
Figure 4
Effect of remibrutinib and rilzabrutinib on bleeding time in vitro. Citrate anticoagulated blood samples were pre-incubated for 1 h at 37°C with solvent (DMSO, 0.1%) or increasing concentrations of remibrutinib or rilzabrutinib and then transferred to collagen/epinephrine cartridges. The in vitro closure time (CT) was measured with the PFA-200. DMSO (1) and DMSO (2) control samples were measured at the beginning and end of the experiment, respectively. (A) Representative PFA-200 tracings. (B) The aligned dot plot bar charts show CT values of different concentrations of remibrutinib and rilzabrutinib. Values are mean ± SD (n = 6). Statistical analysis was carried out using the Wilcoxon matched-pairs signed rank test comparing against DMSO1 (*p < 0.05) or concentrations of remibrutinib (0.1 μM) and rilzabrutinib (0.5 μM) that inhibited Btk-dependent pathways of platelet aggregation by >90% (#p < 0.05).
For rilzabrutinib it was found that a concentration of 0.2 μM which inhibited GPVI-dependent plaque-stimulated platelet aggregation by 56% (Figure 1B) did not affect significantly the closure time. A concentration of 0.5 μM rilzabrutinib equipotent to 0.1 μM remibrutinib suppressed >90% Btk-dependent platelet aggregation after low dose collagen- and ristocetin-stimulated aggregation (Table 1; Figure 2) and significantly increased closure time by 67% (Figures 4A,B). The closure time was significanly more prolonged than by 0.1 μM remibrutinib (Figure 4B). A concentration of 1 μM rilzabrutinib prolonged bleeding time maximally. DMSO, the solvent of BTKi, did not affect closure time as shown previously (9), and the DMSO controls showed similar values at the beginning and the end of the experiments (Figures 4A,B).
Table 1
| BTK Inhibitors | IC50 (μM) | Therapeutic drug plasma level (μM) |
|---|---|---|
| Remibrutinib | 0.03* | 0.46a |
| Rilzabrutinib | 0.16* | 0.33b |
| Fenebrutinib | 0.016* | 0.6c |
| Ibrutinib | 0.025# | 0.31d |
| Zanubrutinib | 0.094# | 1.4e |
| Tirabrutinib | 0.268# | 1.96f |
| Acalabrutinib | 0.372# | 1.78g |
| Evobrutinib | 1.20# | Not known |
IC50 values of remibrutinib, rilzabrutinib and other BTK inhibitors for inhibition of low degree GPVI stimulated platelet aggregation, and comparison with therapeutic drug plasma levels.
Hirudin-anticoagulated blood was pre-incubated with the BTKi for 1 h or 15 min (fenebrutinib, Supplementary Figure 1) prior to stimulation with plaque homogenate.
Hirudin-anticoagulated blood was pre-incubated with the BTKi for 1 h before stimulation with low collagen concentrations (0.2–0.5 μg/ml). Platelet aggregation was measured by multiple electrode aggregometry (MEA).
Remibrutinib, 100 mg q.d, optimal dose in phase I study (38).
Rilzabrutinib, 300 mg b.i.d (39).
Fenebrutinib, 200 mg q.d (40).
Ibrutinib, 420 mg q.d (41).
Zanubrutinib, 320 mg q.d (42).
Tirabrutinib, 320 mg q.d (43).
Acalabrutinib, 100 mg b.i.d (44).
Discussion
We demonstrate here in our study that (i) remibrutinib and rilzabrutinib inhibit and delay dose-dependently atherosclerotic plaque-induced GPVI-mediated platelet aggregation; (ii) remibrutinib (0.1 μM) and rilzabrutinib (0.5 μM) also block Btk-dependent GPVI-, GPIb/VWF- and FcγRIIa-stimulated platelet aggregation; (iii) higher concentrations of remibrutinib (≥0.2 μM) and therapeutic concentrations of rilzabrutinib (≥0.2 μM) prolong the bleeding time in vitro as measured by PFA-200.
According to the dose-response curve (Figures 1A,B), the potency for platelet inhibition of low degree GPVI-induced platelet aggregation of remibrutinib (IC50 = 0.03 μM) was 5 times higher than that of rilzabrutinib (IC50 = 0.16 μM). Compared with other BTKi (Table 1), remibrutinib is only slightly less potent than fenebrutinib (IC50 = 0.016 μM) and ibrutinib (IC50 = 0.025 μM) and more potent than zanubrutinib, rilzabrutinib, tirabrutinib, acalabrutinib and evobrutinib. The IC50 values of remibrutinib (IC50 = 0.03 μM) and rilzabrutinib (IC50 = 0.16 μM) are 12-times and 2-fold lower than the optimal plasma levels as determined in clinical phase 1 studies, respectively (38, 39). Additionally, both inhibitors induced a dose-dependent increase in delay of atherosclerotic plaque-induced aggregation that was associated with the suppression of aggregation in blood (Figure 1C). A delay was also shown in a previous study using ibrutinib- and acalabrutinib-treated washed platelets stimulated by collagen while the maximal aggregation was unaffected (17).
Remibrutinib (0.1 μM) and rilzabrutinib (0.5 μM) significantly suppressed by >90% GPVI-dependent aggregation on low dose collagen, GPIb/VWF-dependent aggregation on ristocetin stimulation, and FcγRIIA-dependent aggregation upon CD32 cross-linking, but it had no effect on TRAP, AA, or ADP stimulation as expected according to the results of previous studies with other BTKi (7, 9, 16, 17), although it has to be stated that a non-existing effect is difficult to prove and may depend on the experimental conditions.
High dose collagen GPVI-dependent aggregation was suppressed to a similar degree of about 30% with remibrutinib (0.1 μM), rilzabrutinib (0.5 μM) and the Btk-selective reversible BTKi fenebrutinib (0.1 μM) (Supplementary Figure 2). This may indicate that the concentrations and incubation conditions of remibrutinib and rilzabrutinib used are selective for inhibition of Btk and unlikely to also inhibit Tec in platelets. This is unexpected considering the potent inhibition of Tec by rilzabrutinib in vitro (22). Rilzabrutinib by inhibiting Tec in addition to Btk would have shut-off GPVI signaling after high collagen stimulation.
As shown in several studies, low-degree GPVI activation only depends on Btk, while high dose collagen-induced GPVI signaling is also dependent on Tec co-activation (9, 15, 19, 45). In a previous study, 50 nM fenebrutinib was applied and only suppression of platelet aggregation on low but not high dose collagen stimulation was observed (9). Our different results may be explained due to the higher concentration of fenebrutinib (0.1 μM) applied in our study providing a more complete inhibition of Btk.
Our results show that the remibrutinib concentration to fully inhibit Btk-dependent pathways of platelet aggregation (0.1 μM) is lower than the reported maximal plasma level (0.46 μM) in a phase I study after intake of 100 mg q.d. for 12 days (38). Thus, this concentration is expected to block completely Btk-dependent signaling in platelets in vivo. The equivalent rilzabrutinib concentration (0.5 μM) is higher than the plasma Cmax reported in clinical studies after therapeutic dosage for autoimmune diseases (0.33 μM) (Table 1) (39). Since the IC50 of rilzabrutinib for inhibition of plaque-induced platelet aggregation in blood was lower (0.16 μM), it is likely that therapeutic concentrations of rilzabrutinib inhibit Btk-dependent pathways of platelet aggregation, but not entirely. Our results are in contrast to findings showing no inhibition of ristocetin- and high dose collagen- induced aggregation of platelet-rich plasma from healthy donors and ITP patients pre-incubated with 1 μM rilzabrutinib for 15 min in vitro (26, 46). The discrepancy might be explained by differences of the experimental system used (blood vs. PRP), different concentrations of collagen (low vs. high) and exposure times of rilzabrutinib (long vs. short). We selected a long exposure time (1 h), since this might better simulate the in vivo situation after absorption of the drug, and previous studies have shown that platelet inhibition with irreversible BTKi increases with the exposure time (17, 19).
Bleeding is a frequent side effect of treatment with certain irreversible BTKi such as ibrutinib and the second generation BTKi acalabrutinib, zanubrutinib, and tirabrutinib used to treat B-cell malignancies (5, 47–49). Exclusive inhibition of Btk should not increase bleeding since XLA patients who are deficient of Btk do not show an impairment of haemostasis (13). It has been discussed that bleeding by these BTKi is related to off-target inhibition of Tec, since this kinase is functionally involved in GPVI-induced platelet activation (8, 15). By comparison, for fenebrutinib, a reversible highly selective BTKi, which is the most selective BTKi and which shows no inhibition of Tec (50), no bleeding events were reported in clinical trials (non-Hodgkin lymphoma, chronic lymphocytic leukemia, rheumatoid arthritis, and systemic lupus erythematosus) (5). Also, fenebrutinib in vitro, even at very high concentrations up to 1 μM did not prolong bleeding time measured by the PFA-200 (9).
The reversible BTKi fenebrutinib binds to an inactive conformation of Btk (51). Also, remibrutinib which was developed from fenebrutinib-like scaffolds to bind to the inactive conformation of Btk (20, 51) showed a 175-fold higher affinity for Btk over Tec in binding assays in vitro (20). Thus, it was expected that remibrutinib would not increase in vitro bleeding time measured by PFA-200, similar to fenebrutinib (9). However, we observed that bleeding times in vitro were already slightly but significantly increased after blood incubation with 0.1 μM remibrutinib (which inhibited >90% of Btk-dependent pathways of platelet aggregation), and strongly prolonged by remibrutinib concentrations of 0.2 and 0.5 μM. The results for remibrutinib are similar to a previous study, in which low concentrations of the irreversible BTKi ibrutinib, zanubrutinib, acalabrutinib, and tirabrutinib inhibited GPVI- dependent platelet aggregation by >70%, but 2- to 2.5-fold higher concentrations of these BTKi were required to significantly increase the bleeding time in vitro (19). The increase of closure time was similar to that observed after treatment with low dose aspirin (52).
In a phase I placebo controlled clinical trial of remibrutinib (total 156 healthy subjects), mild self-limited bleeding events were observed only in 4 persons in the multiple-ascending dose cohorts with remibrutinib intake for 12 days. These included two subjects in the 600 mg q.d. cohort with epistaxis and two subjects in the 100 mg cohort with trauma-triggered hematomas (38).
Rilzabrutinib in our study slightly but non-significantly increased at 0.2 μM closure time in the PFA device, the increase was at 0.5 μM pronounced (Figure 4B). Potent Tec inhibition could contribute to the increased in vitro bleeding time (5); however, the results of the aggregation studies upon stimulation with high concentrations of collagen argue against simultaneous Tec inhibition in platelets by 0.5 μM of rilzabrutinib (see above).
Thus, the mechanisms underlying the increase of closure times elicited by remibrutinib as well as rilzabrutinib are unlikely to involve off-target inhibition of Tec. They could be related to effects on the Btk protein itself. Recently it was found that binding of certain irreversible BTKi (except fenebrutinib) to the kinase domain had long-range allosteric effects on the SH2-and SH3- regulatory domains changing their conformation toward an activated state of the protein (53).
In contrast to remibrutinib, there was not a clear difference of rilzabrutinib concentrations that inhibited Btk-dependent pathways of platelet aggregation in the MEA and robustly increased the closure time in the PFA; the concentration of rilzabrutinib of 0.5 μM does both. Maximal therapeutic concentrations of rilzabrutinib (0.33 μM) are expected to significantly increase the closure time in the PFA device, but no treatment-related bleeding had been noted in the ITP clinical trial with rilzabrutinib (25), although the median platelet count at study entry was only 14.173/μl (25). However, 7% (2/27) of patients treated with rilzabrutinib had treatment-related epistaxis as observed in the latest pemphigus clinical trial (24).
Limitations
Although our in vitro study has the advantage of reducing the complexity of the experimental conditions, and the different effects of the two BTKi studied on platelets in blood are obvious, these data cannot directly be translated into the situation in vivo. Clinical studies of platelet function ex vivo after oral intake of therapeutic dosage are warranted to approach the in vivo effects of remibrutinib and rilzabrutinib on platelets.
Conclusion
In the present study we found significant differences of the two BTKi remibrutinib and rilzabrutinib on platelets that would favor remibrutinib as a candidate for further development as an antiplatelet drug to inhibit Btk-dependent platelet activation pathways underlying atherothrombosis and certain platelet-related immune disorders. Since de novo protein synthesis in platelets is very limited and because low concentrations of irreversible BTKi such as remibrutinib may covalently inactivate platelet BTK already by a single exposure at low concentrations during absorption, it is likely that low doses of such a selective irreversible BTKi are effective in cardiovascular prevention without affecting the immune system (7, 8, 54). Our study further suggests that off-target effects on Tec are unlike to be involved in the increase of closure time measured by PFA, and may not explain the bleeding side effects elicited by BTKi.
Funding
This work was supported by the Deutsche Forschungsgemeinschaft, SFB1123, A2 (PH); RD was sponsored by the Ludwig-Maximilians-University (LMU)-China Scholarship Council (CSC) program.
Publisher's Note
All claims expressed in this article are solely those of the authors and do not necessarily represent those of their affiliated organizations, or those of the publisher, the editors and the reviewers. Any product that may be evaluated in this article, or claim that may be made by its manufacturer, is not guaranteed or endorsed by the publisher.
Statements
Data availability statement
The original contributions presented in the study are included in the article/Supplementary Material, further inquiries can be directed to the corresponding author/s.
Ethics statement
The studies involving human participants were reviewed and approved by Ethics Committee of the Faculty of Medicine of the University of Munich. Written informed consent for participation was not required for this study in accordance with the national legislation and the institutional requirements.
Author contributions
RD designed and performed experiments, analyzed data, and wrote the manuscript. LG performed experiments and analyzed data. RB provided plaque material. MS supervised experiments and contributed to discussions. CW supervised and contributed to discussions. WS conceived the study, designed experiments, and wrote the manuscript. PH supervised and analyzed experiments and wrote the manuscript. All authors have contributed significantly to this manuscript.
Conflict of interest
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
Supplementary material
The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fcvm.2021.749022/full#supplementary-material
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Summary
Keywords
atherothrombosis, platelet-aggregation, bleeding, PFA, MEA
Citation
Duan R, Goldmann L, Brandl R, Spannagl M, Weber C, Siess W and von Hundelshausen P (2021) Effects of the Btk-Inhibitors Remibrutinib (LOU064) and Rilzabrutinib (PRN1008) With Varying Btk Selectivity Over Tec on Platelet Aggregation and in vitro Bleeding Time. Front. Cardiovasc. Med. 8:749022. doi: 10.3389/fcvm.2021.749022
Received
28 July 2021
Accepted
31 August 2021
Published
24 September 2021
Volume
8 - 2021
Edited by
Rory R. Koenen, Maastricht University, Netherlands
Reviewed by
Owen McCarty, Oregon Health and Science University, United States; Dominik Rath, Tübingen University Hospital, Germany
Updates
Copyright
© 2021 Duan, Goldmann, Brandl, Spannagl, Weber, Siess and von Hundelshausen.
This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Philipp von Hundelshausen Philipp.von_Hundelshausen@med.uni-muenchen.de
This article was submitted to Atherosclerosis and Vascular Medicine, a section of the journal Frontiers in Cardiovascular Medicine
Disclaimer
All claims expressed in this article are solely those of the authors and do not necessarily represent those of their affiliated organizations, or those of the publisher, the editors and the reviewers. Any product that may be evaluated in this article or claim that may be made by its manufacturer is not guaranteed or endorsed by the publisher.