Bruton’s Tyrosine Kinase Inhibitors Impair FcγRIIA-Driven Platelet Responses to Bacteria in Chronic Lymphocytic Leukemia

Bacterial infections are a major cause of morbidity and mortality in chronic lymphocytic leukemia (CLL), and infection risk increases in patients treated with the Bruton’s tyrosine kinase (Btk) inhibitor, ibrutinib. Btk and related kinases (like Tec) are expressed in non-leukemic hematopoietic cells and can be targeted by ibrutinib. In platelets, ibrutinib therapy is associated with bleeding complications mostly due to off-target effects. But the ability of platelets to respond to bacteria in CLL, and the potential impact of ibrutinib on platelet innate immune functions remain unknown. FcγRIIA is a tyrosine kinase-dependent receptor critical for platelet activation in response to IgG-coated pathogens. Crosslinking of this receptor with monoclonal antibodies causes downstream activation of Btk and Tec in platelets, however, this has not been investigated in response to bacteria. We asked whether ibrutinib impacts on FcγRIIA-mediated activation of platelets derived from CLL patients and healthy donors after exposure to Staphylococcus aureus Newman and Escherichia coli RS218. Platelet aggregation, α-granule secretion and integrin αIIbβ3-dependent scavenging of bacteria were detected in CLL platelets but impaired in platelets from ibrutinib-treated patients and in healthy donor-derived platelets exposed to ibrutinib in vitro. While levels of surface FcγRIIA remained unaffected, CLL platelets had reduced expression of integrin αIIbβ3 and GPVI compared to controls regardless of therapy. In respect of intracellular signaling, bacteria induced Btk and Tec phosphorylation in both CLL and control platelets that was inhibited by ibrutinib. To address if Btk is essential for platelet activation in response to bacteria, platelets derived from X-linked agammaglobulinemia patients (lacking functional Btk) were exposed to S. aureus Newman and E. coli RS218, and FcγRIIA-dependent aggregation was observed. Our data suggest that ibrutinib impairment of FcγRIIA-mediated platelet activation by bacteria results from a combination of Btk and Tec inhibition, although off-target effects on additional kinases cannot be discarded. This is potentially relevant to control infection-risk in CLL patients and, thus, future studies should carefully evaluate the effects of CLL therapies, including Btk inhibitors with higher specificity for Btk, on platelet-mediated immune functions.

Introduction

Chronic lymphocytic leukemia (CLL) is the most common form of leukemia in the Western World, with approximately 3750 new cases diagnosed annually in the United Kingdom (1). Infectious complications are a major cause of morbidity and mortality in CLL patients (2, 3). The increased risk of infection is due to multiple factors including inherent disease-related immune dysfunction due to secondary hypogammaglobulinemia and T-lymphocyte dysfunction; patient-related factors like age, frailty and co-morbidities; and therapy-related immunosuppression (4).

Bruton’s tyrosine kinase (Btk) is a member of the Tec family of cytoplasmic tyrosine kinases, with a primary role in CLL pathogenesis through signaling downstream of the B cell receptor (BCR) (5). The first-generation inhibitor of Btk (iBtk), ibrutinib, is an effective therapeutic strategy for CLL but has significant toxicity, particularly related to infections and hemorrhagic complications (5–8), due to inhibition of Btk expressed in other (non-B lymphocyte) hematopoietic cells and off-target effects on other kinases (9–11). Bleeding complications are linked to ibrutinib inhibition of platelet responses to multiple agonists that specifically signal through tyrosine kinase-linked receptors, including GPVI, GPIb-IX-V, CLEC-2, and integrins αIIbβ3 and α2β1 (12–16). Healthy individuals and CLL patients can be classified in two groups characterized by low or high platelet sensitivity to ibrutinib based on collagen-induced platelet aggregation in vitro, which is related to drug efflux pumps (17). However, a recent study suggests that ibrutinib-dependent bleeding in CLL patients also involves underlying disease-related changes in platelets including decreased platelet count and impaired platelet response to ADP (18).

Platelets play important immune functions during infection like scavenging and containment of bacteria, secretion of antimicrobial substances and interaction with leukocytes (19–24). In CLL, alterations in the innate immune system have been reported, including impaired function of neutrophils, natural killer cells and monocyte/macrophages (4, 25, 26), however, platelet immune functions remain uncharacterized. Moreover, the potential effect of iBtk therapy on platelet responses to infection has not been addressed. Streptococcus pneumoniae and Haemophilus influenzae are predominant pathogens in CLL, however, ibrutinib treatment has also been associated with serious infections by Staphylococcus aureus and Escherichia coli (3, 6, 27, 28). Importantly, most of these bacterial species are known to cause platelet activation (29–32). When platelets encounter bacteria, contact among them usually involves multiple bacterial strain-specific interactions with different platelet receptors [e.g., FcγRIIA (also known as CD32a), αIIbβ3, GPIb, complement receptor gC1q-R, and Toll-like receptor 2] (33, 34). Although each one of these molecular interactions can contribute to the adhesion and/or platelet activation steps, FcγRIIA has a central role in triggering final platelet activation in response to a wide range of bacteria (29–31).

FcγRIIA recognizes IgG-opsonized pathogens and signals via its cytoplasmic immunoreceptor tyrosine-based activation motif domain (30). Ligation of FcγRIIA by antibody crosslinking causes phosphorylation of Btk and Tec in healthy donor platelets (35) and leads to platelet activation that can be inhibited by iBtks (36). However, activation of FcγRIIA by bacteria is different from crosslinking the receptor with antibodies (29–31). Distinct features of the former include the presence of a lag phase between stimulation and onset of aggregation, and the fact that FcγRIIA phosphorylation and platelet secretion depend on integrin αIIbβ3 engagement (29, 31). Therefore, it is necessary to study the effect of iBtks on platelet FcγRIIA activation following exposure to pathophysiological stimuli including bacteria.

In this study, we analyze if platelets from CLL patients can respond to bacteria in an FcγRIIA-dependent manner and investigate the hypothesis that ibrutinib impairs such responses potentially contributing to the increased risk of infection reported in CLL patients treated with this drug.

Material and Methods

Reagents

See Supplementary Information for details.

Bacterial Culture and Preparation

S. aureus Newman (a gift from Prof Steve Kerrigan, RCSI, Ireland) and E. coli RS218 (a gift from Prof Ian Henderson, University of Queensland, Australia) were cultured and prepared as described (29, 31) (Supplementary Information).

Human Samples and Ethical Considerations

This study was performed in accordance with relevant ethics committees: Hull York Medical School (reference number 1501) and UK National Health Service Research Ethics (08/H1304/35). Informed consent was obtained from all participants.

Peripheral blood from CLL and X-linked agammaglobulinemia (XLA) patients was taken at the Departments of Haematology and Immunology & Allergy, respectively, at Castle Hill Hospital (Cottingham, UK). Blood was drawn using sodium citrate or acid-citrate-dextrose (ACD) vacutainers (see below), and shipped to the University of Hull within 4 hours of venepuncture for immediate testing. Ibrutinib-treated CLL patients were taking a daily dose of 420 mg, except for two patients who were taking 140 mg. Blood from healthy donors was collected at the University of Hull in syringes containing sodium citrate or ACD from volunteers over 18 years of age not treated with concurrent anti-platelet agents.

Platelet-rich plasma (PRP) and platelet-poor plasma (PPP) were obtained from sodium citrated blood, while washed platelets (WP) were prepared from blood in ACD, as detailed in Supplementary Information.

Platelet Aggregation

Platelet aggregation in PRP or WP was done under stirring conditions (1000 rpm) at 37°C using light transmission aggregometry with a CHRONO-LOG 490 aggregometer (CHRONO-LOG, Havertown, PA, USA). WP reactions were supplemented with 1 mg/ml human fibrinogen and 0.2 mg/ml human IgGs before experimentation. Platelets were stimulated with bacteria and other agonists, including crosslinked collagen-related peptide (CRP-xl), thrombin receptor activator peptide 6 amide (TRAP-6) and ADP. To crosslink FcγRIIA, platelets were incubated with anti-FcγRIIA monoclonal antibody (mAb) (4 μg/ml, clone IV.3) for 2 minutes, followed by the addition of crosslinking F(ab’)₂ rabbit anti-mouse IgG (30 μg/ml), altogether designated as IV.3-xl hereafter.

Platelet Factor 4 Secretion

Supernatants from light transmission aggregometry reactions were collected and analyzed for human platelet factor 4 (PF4) by enzyme-linked immunosorbent assay (ELISA) (R&D Systems), as described in Supplementary Information (29).

Platelet Scavenging and Spreading

PRP samples diluted to 2x10⁷ platelets/ml including 15% autologous plasma were incubated for 1 hour with S. aureus Newman or fibrinogen immobilized on glass coverslips. Cells were stained with Hoechst 33342 (to visualize bacteria) and TRITC phalloidin (to visualize platelets) and imaged using a Zeiss Axio Observer fluorescence microscope equipped with ApoTome structured illumination and an AxioCam 506 camera (Zeiss, UK). See Supplementary Information for details.

Flow Cytometry

Flow cytometry was performed in PRP samples using a BD LSR Fortessa cell analyzer (BD Biosciences) as described in Supplementary Information. Data were analyzed using the FlowJO software (BD Biosciences).

Phospho-Tec ELISA

WP (10x10⁸/ml) supplemented with 1 mg/ml fibrinogen plus 0.2 mg/ml hIgGs were stimulated as required in aggregation conditions. Samples were lysed 3 minutes after the start of aggregation, or at a parallel time point in the case of samples where inhibitors blocked aggregation, by adding an equal volume of 2x lysis buffer (29) and analyzed using a RayBio human phosphotyrosine Tec ELISA kit (RayBiotech. Georgia, USA) following the manufacturer’s instructions.

Western Blot

Protein detection in whole platelet lysates was done by SDS-PAGE and near-Infrared Western Blot Detection (LI-COR Biosciences) using lysates collected from PRP samples in the absence of αIIbβ3 inhibitors, as previously described (29) with minor modifications (see Supplementary Information for details).

Statistical Analysis

GraphPad Prism was used to perform the statistical analysis, including normality Kolmogorov-Smirnov and Shapiro-Wilk tests. Data are presented as the mean ± SD. In case of comparisons between two groups, means were evaluated using Student t-test or Mann-Whitney U test, for parametric and non-parametric data, respectively. If more than two groups were considered, one-factor or two-factor analysis of variance (ANOVA) or Kruskal-Wallis test (for parametric and non-parametric data, respectively) followed by multiple comparison tests were performed. For categorical variables, p values were calculated using the chi-square test or Fisher’s exact test. P ≤ 0.05 was considered significant.

Results

CLL Patients’ Characteristics

A total of 34 untreated and 32 ibrutinib-treated CLL patients were enrolled with their characteristics summarized in Table 1. The median age was 72 years, and most patients received concurrent medications for co-morbidities (Supplementary Table 1). The median number of drugs excluding ibrutinib was four for ibrutinib-treated, and three for untreated patients (Supplementary Table 2). Antiplatelet and anticoagulants were present in 6% of ibrutinib-treated (e.g., aspirin) and 18% of untreated (e.g., aspirin, clopidogrel, warfarin) CLL patients (Supplementary Table 1). Notably, 59% of ibrutinib-treated patients were taking prophylactic antibiotics, and 13% were on combined chemotherapy (venetoclax).

TABLE 1

Table 1 Characteristics of chronic lymphocytic leukemia patients enrolled in the study.

CLL Patients Taking Ibrutinib Have Impaired Platelet Activation in Response to FcγRIIA Crosslinking and Bacteria

Bacteria interact with plasma proteins (including IgGs) and platelet receptors in a bacterial strain-specific manner (34). S. aureus Newman and E. coli RS218 are known to cause IgG-dependent FcγRIIA-mediated aggregation and granule secretion in platelets derived from healthy donors (29, 31). Therefore, we asked whether platelets from CLL patients would be similarly responsive to bacteria and, if so, whether ibrutinib treatment would interfere with platelet immune functions. We tested platelet activation induced by clustering of FcγRIIA via IV.3-xl, bacteria, and GPVI-specific agonist, CRP-xl, in the presence of plasma. We also stimulated platelets with TRAP-6 and ADP, which are agonists for G-protein coupled receptors that are not affected by ibrutinib (12–14).

Platelets derived from untreated CLL patients responded to FcγRIIA crosslinking (IV.3-xl) and CRP-xl at levels comparable to controls (Figure 1A). S. aureus Newman and E. coli RS218 induced full or nearly full aggregation in 8 and 9 out of 13 samples respectively, similarly to TRAP-6 and ADP, with aggregation to S. aureus Newman and TRAP-6 being significantly lower than in controls (Figure 1A). The antiplatelet agent, clopidogrel, was taken by two CLL patients, but their platelets aggregated fully to bacteria; however, two aspirin-treated CLL patients showed a reduction in aggregation to bacteria, especially S. aureus Newman (Supplementary Figure 1).

FIGURE 1

Figure 1 CLL platelet aggregation and secretion in response to bacteria and IV.3 mAb mediated FcγRIIA crosslinking are impaired in CLL patients taking ibrutinib. (A) Characterization of platelet aggregation responses in healthy controls (n=17-18), untreated (n=13) and ibrutinib-treated (n=16-17) CLL patients. PRP samples were stimulated with crosslinked IV.3 mAb (IV.3-xl; 4 μg/ml mAb IV.3 followed by 30 μg/ml F(ab’)2 rabbit anti-mouse IgG), S. aureus Newman, E. coli RS218, 3 μg/ml CRP-xl, 3 μM TRAP-6, or 10 μM ADP. Aggregation was recorded by light transmission aggregometry. Reactions were run for 20 minutes from onset of aggregation for IV.3-xl and bacteria, and 10 minutes for the rest of agonists, and maximum aggregation was calculated. (B) Characterization of α-granule secretion in ibrutinib-untreated (n=13) and treated (n=15-16) CLL patients. Supernatants from PRP aggregation reactions were collected at 20 minutes of onset of aggregation for IV.3-xl and bacteria, and 10 minutes in the case of other agonists. Levels of PF4 as a marker of α-granule secretion were measured by PF4 ELISA. (C) Lag time for onset of platelet aggregation in response to bacteria. For healthy donor and ibrutinib-untreated platelet samples, the lag time for onset of aggregation (e.g., time between bacteria injection and start of platelet aggregation) was calculated in those cases in which aggregation took place in response to S. aureus Newman (healthy controls, n=18; CLL, n=11) and E. coli RS218 (healthy controls, n=17; CLL, n=11). (D) Effect of FcγRIIA and Src inhibition on ibrutinib-untreated CLL platelet aggregation. PRP samples (n=10-12) were incubated with 4 μM dasatinib (Src inhibitor) for 2 min, 20 μg/ml IV.3 mAb (FcγRIIA inhibitor) for 10 minutes, or vehicle before being stimulated with agonists and monitored by light transmission aggregometry. (E) Effect of FcγRIIA and Src inhibition on ibrutinib-untreated CLL platelet α-granule secretion. Supernatants from aggregation reactions above were collected at 20 minutes of onset of aggregation for IV.3-xl and bacteria, and 10 minutes in the case of other agonists. PF4 release was measured by ELISA. Data is shown as mean ± SD. Statistical significance was calculated using two-way ANOVA for (A, B), or one-way ANOVA for (D, E), followed by Tukey’s or Sidak’s multiple comparison correction. An unpaired t-test was performed for (C) (*p ≤ 0.05, **p ≤ 0.01, ***p ≤ 0.001, ****p ≤ 0.0001).

Platelet aggregation to S. aureus Newman and E. coli RS218 is characterized by a lag time between bacterial stimulation and start of aggregation that contrasts with the immediate onset of aggregation caused by IV.3-xl (29, 31). Ibrutinib-untreated CLL platelets in which aggregation in response to bacteria was detected (Figure 1A) showed a statistically significant decrease in lag times compared to controls (Figure 1C). Overall, our data indicates that platelets from ibrutinib-free CLL patients aggregate to bacteria in the presence of autologous plasma, although a trend to decreased aggregation compared to FcγRIIA crosslinking is seen.

In contrast, platelets from ibrutinib-treated CLL patients showed strong inhibition of IV.3-xl-induced aggregation, and a significant decrease in aggregation to bacteria (Figure 1A). As opposed to IV.3-xl, heterogeneity in platelet aggregation to CRP-xl was observed in our ibrutinib-treated platelet group (Figure 1A). In previous studies, defects in collagen-induced platelet aggregation were detected in only a subset of ibrutinib-treated patients (12, 13); and the presence of ibrutinib low and high sensitivity groups of both healthy individuals and CLL patients regarding platelet responses to collagen has been reported (17). As published (12, 13), responses to TRAP-6 and ADP (which signal through G-protein coupled receptors) were mostly unaffected in our ibrutinib-treated group (Figure 1A). Differences in aggregation among the three clinical groups were not due to varying platelet concentrations in PRP samples (Supplementary Figure 2).

We next measured release of PF4, a chemokine that can interact with bacteria directly (29, 37), as a marker of α-granule secretion. PF4 was secreted by ibrutinib-untreated CLL platelets upon IV.3-xl and bacteria stimulation (Figure 1B) to similar levels as healthy controls (Figures 1B and 4C) (29). In contrast, ibrutinib-treated CLL patients showed an inhibitory trend of PF4 secretion in response to bacteria, IV.3-xl and CRP-xl, with the latter two being significantly reduced compared to untreated CLL platelets (Figure 1B). PF4 release in response to TRAP-6 and ADP was not affected by ibrutinib treatment (Figure 1B).

To investigate if the CLL platelet responses observed above were mediated by FcγRIIA, aggregation and secretion were measured after incubating PRP with IV.3 mAb, which without the crosslinking F(ab’)₂ inhibits FcγRIIA activation. Consistent with previous observations in healthy donor platelets (29, 31), CLL platelet aggregation and PF4 secretion to S. aureus Newman and E. coli RS218 were inhibited by IV.3 mAb and by the Src inhibitor, dasatinib (Figures 1D, E).

Thus, our results support that platelet immune recognition of bacteria via FcγRIIA is impaired in CLL patients treated with ibrutinib.

The Ability of Platelets to Scavenge S. aureus Newman Is Impaired by Ibrutinib Treatment in CLL Patients

As innate immune effectors, platelets scan the vasculature and collect bacteria (21). Therefore, we next investigated if CLL platelets retain the capacity to scavenge bacteria and whether this is impaired by ibrutinib. Platelets from healthy controls and CLL patients were found to scavenge S. aureus Newman in the presence of autologous plasma with an average (± SD) of 15 ± 8.5 and 13 ± 11.5 bacteria per platelet (bacteria clusters), respectively (Figures 2A, B). Pre-treatment of PRP samples with the integrin αIIbβ3 inhibitor, eptifibatide, abolished scavenging of bacteria by both control and CLL platelets (Figures 2A, B), pointing out to a key role for the integrin in this response. Scavenging was also dependent upon FcγRIIA (Supplementary Figure 3). Remarkably, platelets from CLL patients taking ibrutinib could bind to S. aureus Newman, but showed no morphological changes indicative of activation as compared to controls and were not able to scavenge bacteria (Figures 2A, B).

FIGURE 2

Figure 2 S. aureus Newman can be scavenged by platelets from ibrutinib-untreated but not ibrutinib-treated CLL patients. PRP samples from healthy controls, ibrutinib-untreated CLL and ibrutinib-treated CLL were adjusted to 2 x10⁷ platelets/ml and 15% autologous plasma. Samples were incubated with eptifibatide (9 μM) to inhibit integrin αIIbβ3 or vehicle for 2 minutes and incubated for 1 hour with S. aureus Newman or fibrinogen immobilized on glass coverslips. Coverslips were then washed, fixed, permeabilized, and stained with Hoechst 33342 (grey color, bacteria staining) and TRITC phalloidin (red color, platelet staining). Coverslips were mounted and visualized by fluorescence microscopy. (A) Representative images are presented, with scale bars showing 20 μm. For S. aureus Newman, arrowheads indicate examples of clusters of bacteria scavenged by platelets, and maximum projections of Z-stack images of individual platelets are included. (B) Platelet interactions with S. aureus Newman. Graphs show number of platelets per surface area (top panel), the percentage of platelets scavenging bacteria (middle panel) and the number of bacteria per cluster (bottom panel). Number of samples per clinical group were as follows: healthy controls, n=7 vehicle and n=5 eptifibatide; CLL, n=9 vehicle and n=6 eptifibatide; ibrutinib-treated CLL, n=6 for both vehicle and eptifibatide. (C) Platelet spreading on immobilized fibrinogen. Graphs show number of platelets per surface area and percentage of platelets with filopodia (finger-like cellular protrusions) and lamellipodia (laterally extended protrusions characteristic of later stages of spreading). Healthy controls, n=8; CLL, n=9, ibrutinib-CLL, n=9. All data is shown as mean ± SD. Statistical significance was calculated using one-way or two-way ANOVA followed by Tukey’s multiple comparison correction (*p ≤ 0.05, **p ≤ 0.01, ***p ≤ 0.001).

The same platelet samples were tested for spreading on immobilized fibrinogen. During spreading, the actin cytoskeleton rearranges causing cellular protrusions including finger-like filopodia and laterally extended lamellipodia; the latter being characteristic of later stages of spreading (38). A statistically significant decrease in total number of CLL platelets binding to fibrinogen was detected compared to healthy controls (Figures 2A, C), however, both groups showed similar percentages of platelets with lamellipodia. In contrast, platelets from CLL patients taking ibrutinib bound to fibrinogen to similar levels as controls, but did not spread (Figures 2A, C), consistent with published studies performed with washed platelets (14, 39). These data show decreased efficiency in platelet bacteria-scavenging ability and spreading in CLL patients treated with ibrutinib.

Changes in CLL Platelet Granularity and Membrane Expression of αIIbβ3 and GPVI, but not FcγRIIA, Are Differentially Dependent on Ibrutinib Treatment

The reduction in platelet responses to bacteria observed in ibrutinib-treated CLL patients could be due to heterogeneity in surface expression of important receptors like FcγRIIA and αIIbβ3 (40). Therefore, we performed flow cytometry analyses of platelets derived from our three clinical groups to measure membrane protein levels of αIIbβ3, FcγRIIA and GPVI in PRP samples (Supplementary Figure 4). This analysis revealed no change in cell size, but a significant decrease in granularity/complexity in untreated CLL platelets (Figure 3A). We also observed significant reductions of αIIbβ3 (as detected by two different mAb clones against CD41, the αIIb subunit) and GPVI, but not FcγRIIA (CD32), in CLL platelets independently of ibrutinib treatment when compared to healthy control platelets (Figure 3B). This suggests that decreased levels of αIIbβ3 in blood circulating platelets are unlikely to be the major or only cause of inhibition of ibrutinib-treated CLL platelet responses to bacteria.

FIGURE 3

Figure 3 Although different in granularity, platelets from ibrutinib-treated and untreated CLL patients similarly reduce membrane expression of αIIbβ3 and GPVI, but not FcγRIIA. PRP samples from healthy donors (n=10), CLL (n=10) and ibrutinib-treated CLL (n=10) patients were diluted to 1 x10⁷ platelets/ml and incubated with monoclonal antibodies against human integrin αIIb (CD41), GPVI and FcγRIIA (CD32) before being analyzed by flow cytometry. (A) Left histograms show size and granularity in gated platelets, respectively as forward (FSC) and side (SSC) scatter, in representative samples. The bar graphs (right) show the distribution of platelet size and granularity across the three experimental groups. (B) Bar graphs show the mean fluorescence intensity (MFI) of CD41, GPVI, and CD32 in gated platelets, across the three experimental groups. For CD41, technical replicates with two different antibody clones (PE-conjugated clone 5B12, FITC-conjugated clone P2) are shown (left panels). Statistical significance was evaluated in ANOVA analyses, followed by Tukey’s multiple comparison correction. Data is presented as mean ± SD. (**p ≤ 0.01, ***p ≤ 0.001).

Ibrutinib and Acalabrutinib Inhibit Healthy Donor Platelet Activation in Response to Antibody-Mediated FcγRIIA Crosslinking and Bacteria

To investigate the direct effect of ibrutinib on platelet response to bacteria, we performed light transmission aggregometry with healthy control PRP stimulated in vitro with different concentrations of ibrutinib (Figure 4A and Supplementary Figure 5A). Pre-incubation with 5µM ibrutinib for 5 minutes significantly inhibited platelet aggregation to S. aureus Newman and E. coli RS218, but did not cause a significant reduction of aggregation in response to CRP-xl or TRAP-6. A lower dose of ibrutinib (2 µM) was able to abolish aggregation to FcγRIIA crosslinking (IV.3-xl) (Figure 4A). Longer pre-incubation times with ibrutinib (20 and 40 minutes) did not significantly reduce the concentration of drug needed to inhibit aggregation to bacteria (data not shown). As internal controls, IV.3 mAb alone (FcγRIIA inhibitor) and dasatinib (Src inhibitor) were used in PRP, and both inhibited aggregation to S. aureus Newman and E. coli RS218, but not TRAP-6 (Supplementary Figure 5C), as previously reported (29, 31). The integrin αIIbβ3 inhibitor eptifibatide, as expected, blocked aggregation in response to all agonists including TRAP-6 (Supplementary Figure 5C) (29, 31).

FIGURE 4

Figure 4 Ibrutinib and acalabrutinib inhibit healthy control platelet activation by bacteria and IV.3 mAb mediated FcγRIIA crosslinking in the presence of plasma. (A) Characterization of the effect of ibrutinib on platelet aggregation. PRP from healthy controls was incubated in vitro with different doses of ibrutinib for 5 minutes before stimulation with the following agonists: crosslinked IV.3 mAb (IV.3-xl; 4 μg/ml IV.3 mAb followed by 30 μg/ml F(ab’)2 rabbit anti-mouse IgG; n=5), S. aureus Newman (n=7), E. coli RS218 (n=7), 3 μg/ml CRP-xl (n=5) and 3 μM TRAP-6 (n=5). Aggregation was measured by light transmission aggregometry. Reactions were run for 20 minutes from onset of aggregation for IV.3-xl and bacteria, and 10 minutes for the rest of agonists, and maximum aggregation was calculated. (B) Characterization of the effect of acalabrutinib on platelet aggregation. PRP from healthy controls was incubated in vitro with different doses of acalabrutinib for 5 min before stimulating with agonists: IV.3-xl (n=5), S. aureus Newman (n=6), E. coli RS218 (n=5), 3 μg/ml CRP-xl (n=5) and 3 μM TRAP-6 (n=5). Aggregation was measured by light transmission aggregometry as above. (C) PRP from healthy controls (n=5) was incubated with vehicle or inhibitors, 9 μM eptifibatide (αIIbβ3 inhibitor), 20 μg/ml IV.3 mAb (to inhibit FcγRIIA), 4 μM dasatinib (Src inhibitor), or iBtks, 5 μM ibrutinib and 15 μM acalabrutinib. Samples were then stimulated with stated agonists. Supernatants from aggregation reactions were collected at 20 minutes of onset of aggregation for IV.3-xl and bacteria, and 10 minutes for TRAP-6. Levels of PF4 as a marker of α-granule secretion were measured by PF4 ELISA. Data is shown as mean ± SD. Statistical significance was calculated using one-way ANOVA followed by Tukey’s multiple comparison correction (*p ≤ 0.05, **p ≤ 0.01, ***p ≤ 0.001, ****p ≤ 0.0001).

The high concentrations of ibrutinib needed to inhibit aggregation in PRP contrasted with previous studies done in washed platelets (12, 14, 16), thus we wondered if binding of ibrutinib to plasma proteins (41) may explain the difference. As seen in Supplementary Figure 6A, washed platelet aggregation in response to S. aureus Newman was inhibited by 0.5 µM ibrutinib, while 0.1 µM ibrutinib was sufficient to inhibit the response to E. coli RS218 and FcγRIIA crosslinking (IV.3-xl). A higher dose of ibrutinib (1 µM) was necessary to inhibit washed platelet aggregation stimulated with CRP-xl. None of the ibrutinib concentrations tested in PRP and washed platelets caused inhibition of TRAP-6 induced aggregation (Figure 4A and Supplementary Figures 5A, 6A).

The second generation iBtk, acalabrutinib, was also assessed for its ability to inhibit platelet responses to bacteria. Like ibrutinib, acalabrutinib binds irreversibly to Btk at C481 and is highly bound to plasma proteins (42, 43). In PRP, 10-15 µM acalabrutinib impaired aggregation after IV.3-xl and bacteria exposure, but not in response to CRP-xl and TRAP-6 (Figure 4B and Supplementary Figure 5B). In washed platelets, the inhibitory effects of acalabrutinib were more prominent. Aggregation to IV.3-xl was inhibited by 5-10 µM acalabrutinib, while for bacteria, 1µM and 10 µM inhibited aggregation upon exposure to E. coli RS218 and S. aureus Newman respectively (Supplementary Figure 6B). Washed platelet aggregation after stimulation with TRAP-6 and CRP-xl was unaffected or only partially inhibited (10 µM) by acalabrutinib respectively (Supplementary Figure 6B), as previously described (17, 44).

Ibrutinib and acalabrutinib also inhibited platelet α-granule secretion (PF4) in response to IV.3-xl and bacteria, but not to TRAP-6 (Figure 4C). As previously reported (29, 31), eptifibatide blocked PF4 release in response to bacteria, but not to IV.3-xl (Figure 4C). Moreover, PF4 release in response to bacteria (but not TRAP-6) was inhibited by blocking FcγRIIA with IV.3 mAb alone (Figure 4C). This confirms previous observations of the interplay between FcγRIIA and αIIbβ3 in mediating platelet activation, including secretion, to bacteria.

Hence, in keeping with the above results from our clinical cohort of ibrutinib-treated CLL patients, iBtks strongly and directly inhibit immune function even in platelets derived from healthy donors.

Bacteria Induce FcγRIIA- and αIIbβ3-Dependent Btk Activation That Is Inhibited by iBtks

We showed that ibrutinib can inhibit platelet immune recognition of bacteria, mediated by FcγRIIA, whilst not impacting on the surface levels of this receptor, thus we sought to investigate downstream intracellular signaling events. The binding of ibrutinib and acalabrutinib to Btk C481 blocks Btk autophosphorylation in Y223 that is critical for its activation (5). FcγRIIA crosslinking with non-physiological agonists induces Btk Y223 phosphorylation (35), yet it remains unknown if this is also critical downstream of bacteria recognition. In healthy donors, phosphorylation of Btk Y223 was detected in PRP after IV.3-xl and bacteria exposure, although at lower levels than those induced by CRP-xl (Figure 5A). For S. aureus Newman and E. coli RS218, inhibition of FcγRIIA (with IV.3 mAb alone) and αIIbβ3 (with eptifibatide) reduced Btk phospho-Y223 signal to basal levels (Figures 5B.1, B.4 and B.5), which indicates that both receptors control Btk activation in response to bacteria, as opposed to CRP-xl (Figures 5B.1, B.2) and TRAP-6 (Figure 5B.6). For all agonists tested, Btk phospho-Y223 was inhibited below basal levels by ibrutinib and acalabrutinib as expected (Figures 5A, B).

FIGURE 5

Figure 5 Platelet stimulation by bacteria or crosslinked IV.3 mAb causes Btk activation in healthy donors and CLL patients that is inhibited by ibrutinib and acalabrutinib. Phosphorylation of Btk at Y223 was measured by immunoblotting in whole cell lysates collected from healthy control or CLL PRP aggregation reactions using the following agonists: 3 μg/ml CRP-xl, crosslinked IV.3 (IV.3-xl; 4 μg/ml mAb IV.3 followed by 30 μg/ml F(ab’)2 rabbit anti-mouse IgG), S. aureus Newman, E. coli RS218, and 3 μM TRAP-6. In some cases, platelet inhibitors were used as indicated below. All lysates were collected at 3 minutes after the start of aggregation, or a parallel time point in samples in which aggregation was inhibited. Lysates were adjusted to an equivalent of 5 x10⁸ platelets/ml as explained in Materials and Methods. (A) Btk pY223 phosphorylation in healthy donor platelets stimulated with assorted agonists. Pooled data from three independent experiments done with different donors is shown on the right-hand side graph as mean ± SD. Data was normalized to GAPDH. On the left, one representative experiment is presented. (B) Effect of platelet inhibitors on Btk pY223 phosphorylation in healthy control platelets. Before adding agonists, PRP was pre-incubated with either vehicle, 9μM eptifibatide (αIIbβ3 inhibitor, 2 minutes), 20 μg/ml IV.3 mAb (to inhibit FcγRIIA, 10 minutes), or iBtks (5 minutes), 5μM ibrutinib and 15μM acalabrutinib. B.1. Representative images of five independent experiments for CRP-xl, IV.3-xl and S. aureus Newman. B.2 to B.6. Pooled data shown as mean ± SD. Five independent experiments were done for all agonists except for TRAP-6 that was tested four times. Data was normalized to GAPDH. Statistical significance was calculated using one-way ANOVA followed by Tukey’s multiple comparison correction. (C) Ibrutinib dose-response curve for inhibition of Btk Y223 phosphorylation (green) and aggregation (purple) in response to IV.3-xl (n=5) and CRP-xl (n=4). Representative results are shown below the graphs. (D) Btk Y223 phosphorylation in PRP from ibrutinib-untreated (n=5) and treated (n=5) CLL patients stimulated with assorted agonists. Healthy control (HC) samples were included as positive controls. Statistical significance was calculated using one-way or two-way ANOVA followed by Tukey’s multiple comparison correction (*p ≤ 0.05, **p ≤ 0.01, ****p ≤ 0.0001).

We wondered whether signaling through FcγRIIA, rather than GPVI, would be more reliant on Btk activity, and hence sensitive to ibrutinib inhibition. Therefore, we analyzed if there was a correlation between the ibrutinib concentration found to inhibit Btk Y223 phosphorylation and that needed to inhibit aggregation. Upon IV.3-xl, concentrations of ibrutinib that reduced Btk phospho-Y223 to basal levels (1 μM) or below (2 μM) were also able to partially decrease aggregation (Figure 5C), with total inhibition of aggregation requiring higher concentrations of ibrutinib (5 μM). In contrast, inhibition of Btk Y223 phosphorylation did not correlate with suppression of CRP-xl induced aggregation (Figure 5C), as previously reported (16). Thus, phosphorylation of Btk Y223 downstream of bacteria recognition uses both FcγRIIA and integrin pathways, with FcγRIIA potentially being more sensitive to ibrutinib treatment than GPVI, in healthy donor-derived platelets.

We next sought to investigate CLL samples and found that CLL platelets activated Btk in response to IV.3-xl, bacteria, CRP-xl and TRAP-6 to a similar degree as healthy controls (compare Figures 5A, D). This contrasted with ibrutinib-treated CLL platelets in which no phosphorylation of Btk Y223 was detected in response to IV.3-xl, CRP-xl and TRAP-6 (Figure 5D).

Bacteria Induce Platelet Tec Kinase Activation That Is Inhibited by Ibrutinib

Platelets express two members of the Tec family of tyrosine kinases, Btk and Tec. Although Btk has an approximate 8 to 10-fold greater level of expression in human platelets (45), studies suggest that ibrutinib-mediated inhibition of Tec has important consequences in platelet function (14, 16). Thus, we aimed to decipher if Tec activation takes place downstream of FcγRIIA-mediated platelet response to bacteria as seen for IV.3-xl (35). Due to the lack of phospho-specific antibodies to detect Tec autophosphorylation site Y206 (46), total levels of Tec tyrosine phosphorylation were measured by ELISA.

In healthy donor-derived platelets, Tec phosphorylation increased upon exposure to S. aureus Newman and E. coli RS218, and was inhibited by pre-treatment with ibrutinib (Figure 6). Moreover, when CLL platelets were stimulated with S. aureus Newman, Tec phosphorylation reached similar levels as those observed in healthy controls (Figure 6). We used CRP-xl to compare Tec phosphorylation across our three clinical groups. As seen in Figure 6, healthy donor and untreated CLL platelets stimulated with CRP-xl showed an increase in phospho-Tec that was significantly decreased in platelets from ibrutinib-treated patients. Overall, these data suggest that ibrutinib, both at concentrations used in vitro and at therapeutic doses, affects platelet Tec activation.

FIGURE 6

Figure 6 Platelet responses to bacteria involve Tec kinase activation. Characterisation of platelet Tec phosphorylation in healthy controls (n=5), ibrutinib-untreated CLL (n=5) and ibrutinib-treated CLL (n=5) patients. Washed platelets from the three clinical groups were supplemented with fibrinogen and human IgG (commercially available IgGs pooled from healthy donors). Healthy control platelets were incubated in vitro with 5 μM ibrutinib, 15 μM acalabrutinib or vehicle for 5 minutes before adding agonists. Platelet samples were stimulated with either 3 μg/ml CRP-xl, S. aureus Newman or E. coli RS218. Relative phosphorylation of Tec was measured by a phospho-Tec ELISA. Data is shown as mean ± SD. Two-way ANOVA and Sidak’s multiple comparison test were used to compare CRP-xl responses across the three clinical groups. For the effect of ibrutinib on bacteria-induced phospho-Tec in healthy controls, one way ANOVA followed by Tukey’s multiple comparison correction was done. (*p ≤ 0.05, **p ≤ 0.01).

XLA-Derived Platelets Respond to Bacteria in an FcγRIIA-Dependent Manner

Mutations in the Btk gene resulting in lack of Btk expression or function cause XLA, a condition characterized by markedly reduced or absent B cells and profound hypogammaglobulinemia (47). To investigate if Btk function is essential for FcγRIIA-mediated platelet responses to bacteria, we obtained PRP from two XLA patients receiving periodic intravenous immunoglobulin treatment. Platelets from both patients aggregated to S. aureus Newman and E. coli RS218 although with varying lag times (Figure 7A). Upon crosslinking of FcγRIIA (IV.3-xl), no or less aggregation was observed in patients 2 and 1 respectively (Figure 7A), suggesting that this pathway is more strongly affected by Btk deficiency than bacteria-induced activation. Importantly, XLA platelet responses to bacteria were still dependent on FcγRIIA, as aggregation was blocked by pre-incubating PRP with inhibitory IV.3 mAb alone (Figure 7B). Conversely, we detected normal XLA platelet aggregation in response to CRP-xl and TRAP-6 (Figure 7A), which was independent of FcγRIIA (Figure 7B). These results suggest that while Btk has an active role in FcγRIIA-mediated platelet function, this is not essential for FcγRIIA-mediated responses to bacteria.

FIGURE 7

Figure 7 Platelet responses to bacteria can take place in the absence of functional Btk. (A) Characterization of bacteria-induced aggregation of platelets from X-linked agammaglobulinemia patients. PRP samples from two XLA patients were stimulated with crosslinked IV.3 mAb (IV.3-xl; 4 μg/ml IV.3 mAb followed by 30μg/ml F(ab’)₂ rabbit anti-mouse IgG), S. aureus Newman, E. coli RS218, 3 μg/ml CRP-xl, and 3 μM TRAP-6. Aggregation was measured by light transmission aggregometry. (B) PRP from XLA patients was incubated with 20 μg/ml IV.3 mAb (to inhibit FcγRIIA) or vehicle, before stimulation with either S. aureus Newman, E. coli RS218, 3 μg/ml CRP-xl or 3 μM TRAP-6. Aggregation was measured by light transmission aggregometry. Patient 1 (n=3, in different days) had a missense mutation in codon 28 affecting the Btk pleckstrin homology domain, which causes lack of Btk function. Patient 2 (n=1) had a mutation in exon 3 resulting in absence of Btk expression.

Discussion

This study has focused on platelet immune responses in CLL in the context of bacterial infection and ibrutinib therapy. Infectious complications are a major burden in CLL, and the increased risk of infection is multifactorial, including immunosuppression inherent to disease, patients’ age and co-morbidities, and therapy toxicity (3, 4, 6, 27, 28). In CLL, alterations can be found in both the adaptive and innate immune systems, namely T lymphocyte dysfunction, hypogammaglobulinemia, complement defects, and impairment in antimicrobial activity of neutrophils and monocytes (4, 25, 26). Because it is possible that CLL platelets had immune function abnormalities that could be exacerbated by ibrutinib, the first part of our study had two aims: to characterize platelet responses to bacteria in CLL (e.g., in the absence of CLL-targeted treatment) and to investigate the effect of ibrutinib therapy on these responses.

Overall, ibrutinib-untreated CLL platelets responded to S. aureus and E. coli in an FcγRIIA-dependent manner in the presence of autologous plasma, as seen by platelet aggregation, secretion and scavenging of bacteria. We found that platelet scavenging of S. aureus Newman was both FcγRIIA and αIIbβ3-dependent. However, more investigations are needed to further characterize the molecular mechanisms underlying platelet scavenging of pathogens, including potential bacterial-strain specific processes. Previous studies suggest that alternative mechanisms could take place. Gaertner et al. (21) have shown that platelets can scavenge fibrin-bound E. coli and S. aureus, both in vitro and in vivo, boosting the phagocytic activity of neutrophils; while Palankar et al. (22) described a mechanism by which PF4 binding to E. coli promotes antibody opsonization and FcγRIIA-mediated platelet spreading that covers the opsonized bacteria leading to bacterial killing (22). Platelets have also been shown to kill S. aureus Newman, but not S. pneumoniae, in a process that was FcγRIIA independent (23). Moreover, the releasate derived from platelet aggregation can directly kill S. aureus and enhance the antimicrobial function of macrophages (23, 48).

Despite the overall response to bacteria, some variation was observed in ibrutinib-untreated CLL platelets, with some samples not reaching full activation. Differences in bacteria-induced aggregation in healthy donor platelets are not uncommon (49, 50), however, variation in CLL could be due to additional factors like co-morbidities and related medications (51). Indeed, most of our CLL patients were taking multiple medications reflecting a typical population of CLL patients often with multiple comorbidities. The increased bleeding risk found in ibrutinib-treated patients is exacerbated by concurrent intake of antiplatelet or anticoagulant therapy (7), and in vitro studies show that ibrutinib amplifies the effect of cangrelor and indomethacin on platelets (14, 17). However, in our study a minority of patients were taking antiplatelet medications, and thus, future research should be done to investigate the effect of different drug combinations, including iBtk combinations with antiplatelet drugs, on platelet immune functions. Other factors that might explain why platelets from some CLL patients did not activate fully to bacteria are plasma immunoglobulin concentrations (52) and polymorphic variants of FcγRIIA (53, 54). Notably, some of these factors might also account for variable platelet responses to bacteria within healthy individuals (49, 50). Although variations in the expression of FcγRIIA (55) could also affect platelet activation by microorganisms, no significant changes in FcγRIIA levels were detected among our clinical groups.

Three observations suggested alterations in circulating CLL platelets: a decrease in platelet granularity/complexity, an ibrutinib-independent decrease in membrane levels of αIIbβ3 and GPVI compared to controls, and a reduction in lag time for onset of platelet aggregation in response to bacteria; although the latter could also be due to changes in plasma composition in CLL. Our flow cytometry results differ from others in which αIIbβ3 surface expression in CLL platelets was similar to healthy donors (40, 56) but decreased upon ibrutinib treatment (40). Moreover, reduced GPVI levels in CLL platelets were found in one study (56), but not another (40). Platelet alterations could originate during megakaryopoiesis as CLL is characterized by bone marrow dysfunction (57); however, they could also reflect interactions with unknown-disease-related factors once platelets are released into the circulation (57). The modulation of membrane receptor levels can affect platelet reactivity to external stimuli as well as platelet senescence and lifespan (58); and changes in platelet granularity might reflect some degree of activation (with granule centralization) (19). Therefore, future studies are needed to characterize CLL platelet proteomic and structural changes and their potential consequences in platelet function in the presence and absence of iBtks.

A key finding of this investigation is that therapeutic doses of ibrutinib impair platelet responses to S. aureus Newman and E. coli RS218. While it is still possible that an underlying CLL platelet immune dysfunction is significantly worsened by iBtks, the fact that ibrutinib and acalabrutinib also inhibited platelets derived from healthy donors points out to the ability of iBtks to directly interfere with platelet immune functions (independently of additional CLL-specific changes). Despite some conflicting reports regarding the increased risk of infection during ibrutinib therapy in B-cell malignancies, Ball et al. have recently published a systematic review and meta-analysis of randomized controlled trials, including more than 2000 patients, in which a significantly higher risk of infections associated with ibrutinib treatment has been found (6). Ibrutinib inhibition of platelet immune functions might contribute to infection by interfering with the ability of platelets to contain and kill pathogens and crosstalk with other immune cells (19–24, 48, 59); however, this hypothesis will need further evaluation in view of the complex multifactorial nature of infection complications in CLL. For example, ibrutinib affects neutrophil, monocyte and macrophage responses to fungi (10, 11), and these effects might also have important consequences in responses to bacteria. Furthermore, infections cannot be explained by Btk inhibition alone, as seen by the decline in the risk of infection and neutropenia rate over time on ibrutinib therapy presumably due to gradual immune reconstitution (60–62). Notably, in our study some platelet samples from ibrutinib-treated patients aggregated to bacteria, mainly E. coli RS218, suggesting the presence of Btk-independent mechanisms of activation. It is important to point out that immune responses in CLL, including those ones in which platelets might be involved, are likely microorganism dependent. Thus, frequent pathogens like S. pneumoniae, H. influenzae, but also fungi (63) should be examined in this context.

To clarify if newer iBtks with improved selectivity for Btk over other kinases (5, 42, 64) might be beneficial to treat B-cell malignancies, it is important to understand how Btk and structurally related kinases like Tec work in non-malignant cells, including platelets. For this reason, the second part of our study investigated the role of Btk in platelet immunity. Previous studies on healthy donor platelets reported a role for Btk and Tec in FcγRIIA-mediated platelet activation in response to artificial antibody crosslinking and sera from heparin-induced thrombocytopenia patients (35, 36). Here, we studied Btk and Tec activation downstream of bacteria-stimulated platelets from healthy donors and CLL patients. Bacteria and FcγRIIA crosslinking with IV.3 mAb caused Btk activation, and platelet aggregation that was more sensitive to ibrutinib than CRP-xl stimulation, suggesting that Btk has a role downstream of FcγRIIA, as supported by investigations by Goldmann et al. (36). Although the peak plasma concentration of ibrutinib is only 0.3-0.4 μM (65), Btk activation was abolished in platelets derived from ibrutinib-treated patients, which confirmed that therapeutic doses of ibrutinib target platelet Btk. Nonetheless, bacteria also caused platelet Tec phosphorylation that was inhibited by ibrutinib.

Because platelets are anucleated, intracellular signaling studies often rely on animal models. For GPVI, the relative contribution of Btk and Tec in GPVI-mediated platelet activation was studied using platelets from knockout mice, and only those from double Btk and Tec knockout animals were insensitive to CRP-xl (66). However, this strategy is not feasible in the context of our study because murine platelets do not express FcγRIIA, and platelets from FcγRIIA-transgenic mice do not respond to many bacterial strains that are known to activate human platelets, even when supplemented with human IgGs (29). This should be taken as a warning of the limitations of using animal models that lack FcγRIIA to address platelet immune functions that depend on IgGs, thus linking innate and acquired immune responses. Instead, we tested platelets from two XLA patients, which lack functional Btk, and found that they responded to bacteria in an FcγRIIA-dependent manner, although we detected some impairment in aggregation to FcγRIIA crosslinking (IV.3-xl) that will require further investigation. Most commonly, XLA patients suffer from respiratory infections caused by S. pneumoniae and H. influenza. Although S. aureus infections are also reported (67, 68), generally they are not considered significant problems in patients who receive regular immunoglobulin replacement therapy (47), which further suggests that Btk is not essential for the immune system to control infection by specific bacterial species in the presence of normal IgGs. Altogether, and as found for GPVI (15, 35, 66, 69), our results suggest that either Btk is dispensable for platelet aggregation to S. aureus and E. coli, or there is enough Btk/Tec kinase functional redundancy to rescue the activating signaling when Btk is absent. It is also possible that other tyrosine kinases can compensate for the loss of Btk, but still be off-targeted by ibrutinib in CLL patients. Platelet-bacteria interactions are complex and can involve multiple receptor-ligand combinations that are bacterial-strain specific (70), therefore, it is also possible that crosstalk between FcγRIIA/αIIbβ3 and other receptors (e.g., GPIb, complement receptor gC1q-R, and Toll-like receptor 2) (33, 34) and signaling pathways can overcome the absence of Btk.

In summary, this study shows that CLL platelets can respond to S. aureus and E. coli bacteria in an FcγRIIA-dependent manner and provides evidence that ibrutinib impairs such responses. Mechanistically, while FcγRIIA expression was not altered by the treatment, our data demonstrates that ibrutinib inhibits both Btk and Tec kinases downstream of FcγRIIA/αIIbβ3 activation in response to bacteria stimulation. This points out to the importance of evaluating the effect of iBtks used to treat CLL and other hematological malignancies on platelet immune functions.

Data Availability Statement

The raw data supporting the conclusions of this article will be made available by the authors, without undue reservation.

Ethics Statement

The studies involving human participants were reviewed and approved by Hull York Medical School Ethics Committee (Ethics reference number 1501) and UK National Health Service Research Ethics Committee (Ethics reference number 08/H1304/35). The patients/participants provided their written informed consent to participate in this study.

Author Contributions

LN-A designed research, performed most experiments, analyzed data, and wrote the manuscript. AC designed, performed, and analyzed scavenging experiments. ZB and JJ performed experiments. SC designed and supervised flow cytometry research and analyzed data. SK provided access to XLA patients. SH provided key reagents and intellectual input. FR designed and performed platelet scavenging research and analyzed data. DA provided and coordinated access to CLL patients and designed and supervised the study. MA designed and directed research, performed experiments, analyzed data and wrote the manuscript. All authors contributed to the article and approved the submitted version.

Funding

This work was supported by the University of Hull and Hull University Teaching Hospital Trust. LN-A and ARC were recipients of University of Hull PhD scholarships.

Conflict of Interest

DA has received honoraria for speaking from Gilead Pharmaceuticals, funding for conference attendance from Bayer and CSL Behring and research funding from Roche.

The remaining 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.

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.

Acknowledgments

The authors would like to thank Prof. Steven Kerrigan (RCSI, Ireland) and Prof. Ian Henderson (University of Queensland, Australia) for kindly providing S. aureus Newman and E. coli RS218, respectively. We also thank all the patients, healthy donors and staff who participated in the study, and the J. Andrew Grant Fund for Cardiovascular Research for support.

Supplementary Material

The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fimmu.2021.766272/full#supplementary-material

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