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Elevated proportion of TLR2- and TLR4-expressing Th17-like cells and activated memory B cells was associated with clinical activity of cerebral cavernous malformations



Recent evidences have suggested the involvement of toll-like receptor (TLR)-4 in the pathogenesis of cerebral cavernous malformations (CCM). Elevated frequency of TLR+T-cells has been associated with neurological inflammatory disorders. As T-cells and B-cells are found in CCM lesions, the objective of the present study was to evaluate the cytokine profile of T-cells expressing TLR2 and TLR4, as well as B-cell subsets, in asymptomatic (CCMAsympt) and symptomatic (CCMSympt) patients.


For our study, the cytokine profile from TLR2+ and TLR4+ T-cell and B-cell subsets in CCMAsympt and CCMSympt patients was investigated using flow cytometry and ELISA. T-cells were stimulated in vitro with anti-CD3/anti-CD28 beads or TLR2 (Pam3C) and TLR4 (LPS) ligands.


CCMSymptc patients presented a higher frequency of TLR4+(CD4+ and CD8+) T-cells and greater density of TLR4 expression on these cells. With regard to the cytokine profile, the percentage of TLR2+ and TLR4+ Th17 cells was higher in CCMSympt patients. In addition, an elevated proportion of TLR4Tc-1 cells, as well as Tc-17 and Th17.1 cells expressing TLR2 and TLR4, was observed in the symptomatic patients. By contrast, the percentage of TLR4+ IL-10+CD4+ T cells was higher in the CCMAsympt group. Both Pam3C and LPS were more able to elevate the frequency of IL-6+CD4+T cells and Th17.1 cells in CCMSympt cell cultures. Furthermore, in comparison with asymptomatic patients, purified T-cells from the CCMSympt group released higher levels of Th17-related cytokines in response to Pam3C and, mainly, LPS, as well as after activation via TCR/CD28. Concerning the B-cell subsets, a higher frequency of memory and memory activated B-cells was observed in CCMSympt patients.


Our findings reveal an increase in circulating Th17/Tc-17 cell subsets expressing functional TLR2 and, mainly, TLR4 molecules, associated with an increase in memory B-cell subsets in CCM patients with clinical activity of the disease.


Cerebral cavernous malformations (CCM), or cavernous angiomas, are vascular lesions consisting mainly of clusters of grossly dilated brain capillaries presenting altered permeability due to the loss of tight junctions and muscular and elastic tissues, which predisposes patients to increased risk of hemorrhagic stroke, epilepsy and other neurological disorders [1]. CCMs are among the most common vascular malformations of the Central Nervous System (CNS) with an estimated prevalence ranging from 0.4 to 0.9%, mostly detected in adolescents and young adults [2, 3]. Although the majority of CCM cases are sporadic, approximately 20% are inherited as an autosomal dominant trait and, different from sporadic cases, the inherited disease manifests with multiple lesions [1, 4]. In both sporadic and familial cases, CCM results from a mutation at one of three CCM gene loci, CCM1/Krit1, CCM2/MGC4607, and CCM3/PDCD10. These genes encode components of a heterotrimeric intracellular adaptor protein complex, named CCM complex [2,3,4,5], that stabilizes the junctions of endothelial cells by inhibiting overactivation of the MEKK3–KLF2/4 signaling pathway [6, 7]. Despite the knowledge of CCM complex involvement, the severity and natural course of the disease are highly variable, even in patients carrying the same genetic mutations [1,2,3], suggesting the existence of others genetic/epigenetic factors and/or environmental disease modifiers, some of which involving inflammatory mediators, that affect disease outcomes, probably by activating the MEKK–KLF2/4 pathway [8, 9].

The risk of symptomatic CCM has been associated with elevated plasma levels of the pro-inflammatory cytokines interleukin (IL)-1β, IL-2, interferon (IFN)-γ, tumor necrosis factor (TNF)-α and lower concentrations of the anti-inflammatory cytokine IL-10 [10, 11]. In addition, gene polymorphisms expected to increase the expression of membrane CD14 (mCD14) and toll-like receptor (TLR)-4 have been correlated with more severe CCM disease [10, 11]. The mCD14/TLR4 complex forms a pattern recognition receptor classically expressed on monocytes, which is responsible for the recognition of lipopolysaccharides (LPS), a pathogen-associated molecular pattern (PAMP) from Gram-negative bacteria (GNB). Upon LPS engagement, the CD14/TLR4, in association with myeloid differentiation primary response protein 88 (MyD88), activates nuclear factor (NF)-κB, promoting the production of pro-inflammatory cytokines [12, 13]. Interestingly, in experimental model of the disease, LPS, by activating TLR4–MEKK3–KLF2/4 signaling in endothelial cells, accelerated CCM formation in the brain of those animals [14]. Although this study have demonstrated that LPS-induced brain CCM lesions did not depend on were a phenomenon independent of local immune cells, macrophages, B cells and (CD4+ and CD8+) T cells have been observed in perivascular regions of CCM lesions in patients [14]. Moreover, immunocomplexes consisting of IgG and terminal products of complement activation were also detected in CCM lesions [6]. Interestingly, analysis of the complementarity-determining regions 3 (CDR3) sequence of the variable domains of these IgG revealed a local Ig production containing somatic hypermutation into CDR3 regions [6], a genetic event classically dependent on CD4+ T cell help [7, 15].

According to the pattern of secreted cytokines, human effector CD4+ T cells are divided into three major subsets, Th1 (IFN-γ+), Th2 (IL-4+) and Th17 (IL-17+). Th1 cells not only favor macrophage activation by releasing IFN-γ, but also assist CD8+ T lymphocytes differentiation into cytotoxic cells able to kill target cells through the release of perforin and granzymes [16, 17]. Concerning the cytokine pattern, activated CD8+ T cells can be named Tc-1 (IFN-γ+) [18] or Tc-17 (IL-17+) [19]. The signature cytokines produced by Th2 (IL-4) and Th17 (IL-17) cells are implicated in inflammatory processes involving eosinophil and neutrophil activation, respectively [17, 20, 21]. With regard to adaptive humoral immune response, the production of IgG, IgA and IgE neutralizing antibodies classes by activated B cells, and the generation of memory B cells, are dependent on follicular helper T cells (TFH), a CD4+ T cell phenotype identified by the high expression of surface CXCR5 and production of the signature cytokine IL-21 [7, 15]. Although these lymphocytes have been implicated in protection against different pathogens, some effector T cell subsets, mainly those expressing TLR2 and TLR4, are involved in the severity of neurological inflammatory disorders, such as neuromyelitis optic spectrum disorders (NMOSD) [22, 23] and the multiple sclerosis (MS) [24, 25], both autoimmune demyelinating diseases of the CNS. Despite high T cell numbers in CCM lesions, no study has yet been designed to analyze the cytokine profile of these lymphocytes, particularly among T cell subsets expressing TLRs. It is possible that PAMPs may adversely impact the outcome of CCM by favoring the activation of pathogenic TLR+ T cells. Therefore, in the present study, we aimed to evaluate the frequency and cytokine profile of circulating CD4+ and CD8+ T cell subsets expressing TLR2 and TLR4 in asymptomatic and symptomatic CCM patients. Also, we analyzed B cell subsets.



This transversal study included 37 CCM patients, 14 asymptomatic [CCMAsympt, mean age ± SD, 45 ± 13.1 years (7 familial/multifocal, 7 sporadic/solitary)] and 23 symptomatic [CCMSympt, mean age ± SD, 40 ± 13.6 years (3 familial/multifocal, 17 sporadic/solitary)] from the Federal University of Rio de Janeiro and Brazil Cavernoma Alliance. The majority of CCM patients were women (n = 25/37; 10 asymptomatic and 15 symptomatic). Developmental venous anomaly (DVA) was identified in 03 asymptomatic and 09 symptomatic patients. Among symptomatic patients, the clinical manifestations were lesional hemorrhages (87%, n = 20) and seizure crisis (13%, n = 03). We excluded patients who had undergone partial or complete CCM lesion resection or any prior brain irradiation. Except for two patients with epilepsy, who were using Oxcarbazepine (Trileptal) to control their seizure crisis, all other CCM patients recruited were not taking any medication. As the control group (Ctrl), 20 healthy individuals with normal brain Magnetic resonance imaging (MRI) images (10 women and 10 men) (mean age ± SD, 40.1 ± 11.7 years) were also recruited from Federal University of the State of Rio de Janeiro. Subjects with a history of autoimmune disease, neoplasms, smoking, or treatment with psychotropic drugs were excluded, as well as pregnant women. The Ethics Committee for Research on Human Subjects at the Federal University of the State of Rio de Janeiro (UNIRIO, CAAE 69409617.9.0000.5258) approved the study and blood was collected only after written informed consent was obtained from each individual.

Flow cytometry

Mouse anti-human monoclonal antibodies (mAbs) directed against CD3-PerCpCy5.5 (OKT3 clone), CD4-SB600 (SK-3 clone), CD8-FITC (3B5 clone), CD14-APC (61D3 clone), CD16-PE (CB16 clone), CD62L-FITC (Dreg-56 clone), CD45-PE (2D1 clone), CD45RO-PE-Cy7 (UCHL1 clone), TLR2-PE (TL2.1 clone), TLR4-PE (HTA125 clone), CD19-APC (HIB19 clone), CD27-FITC (CLB-27/1 clone), CD38-PE (HIT2 clone), IL-6-PE-Cy7 (MQ2-13A5 clone), IL-10-eFluor450 (JESE-9D7 clone), IL-17-Alexa Fluor 647 (N49-653 clone) and IFN-γ-Alexa Fluor780 (4S.B3 clone), and all isotype control antibodies were purchased from eBioscience (Thermo Fischer scientific, USA). To identify different cytokine-producing T cells subsets [Th1 (CD3+/CD4+ INF-γ+), Tc-1 (CD3+/CD8+ INF-γ+), Th17 (CD3+/CD4+ IL-17+), Th17.1 (CD3+/CD4+ INF-γ+IL-17+), Tc-17 (CD3+/CD8+ IL-17+) and Treg-like cells (CD3+CD4+IL-10+], capable of expressing TLR2 or TLR4, as well as B cells (CD19, CD27, CD38 and IL-10), whole peripheral blood (1 mL) of CCM patients was cultured in a 24-well flat microtiter plate in the absence of stimulus or in the presence of TLR2 ligand [synthetic triacylated lipopeptide (Pam3Csk4—1 μg/ml)] (InvivoGen, San Diego, CA, USA) or TLR4 agonist [LPS (100 ng/ml) from Escherichia coli] (Sigma-Aldrich, St. Louis, MO, USA)]. The TLR concentrations were established in studies conducted by Voo et al. [26]. The cell cultures were kept for 24 h at 37 °C in a humidified 5% CO2 incubator. For cytokine measurement optimization, brefeldin A (10 μg/mL; Sigma-Aldrich) was added 4 h before cell staining with mAbs. Briefly, whole blood cells were incubated with various combinations of mAbs for surface markers (CD3, CD45R0, CD14, CD16, CD4, CD8, TLR2, TLR4, CXCR5, CD19, CD27 and CD38) for 30 min at room temperature in the dark, according to manufacturer's instructions. The cells were washed with PBS + 2% FBS, and then, the whole blood cells were lysed with Fix/Lyse solution (BD Pharmigen, San Diego, USA) for 10 min at room temperature followed by cell permeabilization, which was performed by incubating cells in Cytofix/Cytoperm solution (BD PharMingen, San Diego,) at 4 °C for 20 min. After washing, the mAbs for intracellular cytokine staining (IL-6, IL-10, IL-17, IFN-γ and IL-21) were added in different combinations and incubated for 30 min at 4 °C. To prevent non-specific staining of cells expressing FcRs, FcR blocking reagent was used (Miltenyi Biotec, cat. 130.059.901). The cells were acquired on Attune NxT flow cytometers (Thermo Fisher Corporation) and analyzed using FlowJo software. Isotype control antibodies and single-stained samples were used to periodically check the settings and gates on the flow cytometer. After the acquisition of 100,000–300,000 events, lymphocytes were gated based on forward and side scatter properties after the exclusion of dead cells, using propidium iodide, and doublets.

T cell cultures, cell proliferation and cytokine production

Peripheral blood mononuclear cells (PBMC) from healthy subjects and CCM patients were separated by a Ficoll–Paque gradient, and then submitted to negative selection using magnetic columns to obtain T cells according to manufacturer’s instructions (EasySep ™, cat. 17951, StemCell Technology ™, Vancouver, Canada). Briefly, 50 µL of a cocktail containing monoclonal antibodies directed against B cells, monocytes, dendritic cells and NK cells were added to a 15 mL tube containing approximately 5 × 107 PBMC/mL. After 5 min of incubation, 40 µL/mL of magnetic beads were added to the cell suspension. After rapidly mixing, the cell suspension was incubated at room temperature for 5 min. Subsequently, 4 mL of HBSS were added to the cell suspension and, the tube was placed on the magnet for 5 min. Finally, the supernatants were recovered. The purity of the CD3+ cells was > 98%, as measured by flow cytometry (data not shown). Enriched T cell cultures were then maintained with RPMI-1640 medium supplemented with 2 μM of L-glutamine (GIBCO, Carlsbad, CA, USA), 10% fetal calf serum, 20 U/mL of penicillin, 20 μg/mL of streptomycin and 20 mM of HEPES buffer. In some cultures, Pam3Csk4 (Pam3C, 1 μg/mL) or LPS (100 ng/mL) was added. As a positive control, some T cell cultures were stimulated with anti-CD3/anti-CD28 beads (10 μl/mL). All cell cultures were kept for 48 h at 37 °C and 5% CO2 before evaluation of T cell proliferation and cytokine release. This culture duration was established by our group from time-course T cell proliferation analyzes in response to LPS and Pam3C (data not shown).

The T cell proliferation was measured by [3H] thymidine incorporation added to cultures at 4 μCi/well 8 h prior to the conclusion of the 2-day incubation period. The cells were harvested in glass fibre 8 filters in an automatic cell harvester (Beckman Coulter L56500) and radioactive incorporation was measured using a liquid scintillation counter. The results were shown as stimulation indexes (SI), that is, the mean count per minute (cpm) of stimulated T cells was divided by the mean cpm of unstimulated T cells from the same patient group. An SI > 3 was considered a positive response.

The cytokine levels secreted by the T cells in the supernatants were quantified using OptEIA ELISA kits (BD, Pharmigen, San Diego, CA), according to manufacturer’s instructions. Briefly, each ELISA was performed using pairs of antibodies against IL-6, IL-1β, TNF-α, IL-10, IL-17A (IL-17), IL-21, GM-CSF and IFN-γ. The reaction was revealed with streptavidin–horseradish peroxidase, using 3,3’,5,5’-tetramethylbenzidine (TMB) as substrate. Recombinant human cytokines, at concentrations ranging from 3.5–500 pg/mL, were used to construct standard curves. The plates were read using Multiskan™ FC microplate photometer (Thermo Fischer Scientific).

Statistical analyzes

The statistical analysis was performed using Prism 8.0 software (GraphPad Software). All immunological evaluations were performed in triplicate for each individual and the intra-assay variability ranged from 9.3% to 17.1% (median value of 10.1%) as calculated by the software above. Comparisons between immune assays in cell cultures from the three different groups were performed with ANOVA followed by Tukey test for data with Gaussian distribution and by Kruskal–Wallis followed by Dunn’s test for data without Gaussian distribution. The results were also corrected by Bonferroni. The nonparametric Mann–Whitney U test and the Student’s t test were applied to determine whether the two groups were statistically different for nonparametric and parametric variables, respectively. Significance in all experiments was p < 0.05.


Activated effector CD4+ and CD8+ T cells expressing functional TLR2 and, mainly, TLR4 are expanded in symptomatic CCM patients

For this study peripheral blood was collected from 37 CCM patients, 14 asymptomatic (CCMAsympt, mean ± SD, 45 ± 13.1 years) and 23 symptomatic (CCMSympt, mean ± SD, 40 ± 13.6 years) (Table 1). For control group (Ctrl), blood samples were obtained from 20 healthy subjects. As expected [3], the majority of CCM patients was female and the Sporadic form of disease was dominant. Out of the 23 symptomatic patients, 3 (13%) presented with epilepsy and the other 20 (87%) presented with at least one episode of bleeding. Among the 3 patients with epilepsy, 2 were under pharmacological treatment with oxcarbazepine at the time of blood sampling (Table 1). Despite the use of therapy to control epileptic seizures, these two patients were not excluded, because no difference was observed regarding immunological assays among them and the other symptomatic patients. Developmental venous anomaly (DVA) was identified in 03 asymptomatic and 09 symptomatic patients. The majority of patients and healthy subjects were Caucasians.

Table 1 Features and demographic of CCM patients and healthy subjects

The main objective of this study was to evaluate the expression of TLR2 and TLR4 on (CD4+ and CD8+) T lymphocytes from CCMAsympt and CCMSympt patients, as well as the cytokine profile of these T cell subsets. Taking into account the FSC versus SSC parameters (Additional file 1: Fig. S1A), the frequency of (CD4+ and CD8+) T cells expressing TLR2 and TLR4 in the classical T cell gate was low and showed no difference between healthy subjects (control group) and CCMAsympt or CCMSympt patients (Additional file 1: Fig. S1B). Furthermore, these T cells were negative for IL-6, IL-17, IFN-γ and IL-10 cytokines (data not shown). On the other hand, higher frequency of T cells expressing TLR2 and TLR4 was identified in the gate containing larger and more granular CD45+ cells in blood samples from CCM patients (Additional file 2: Fig. S2A). These T cells were negative for CD14 and CD16 markers, excluding the presence of monocytes and NK cells (Additional file 2: Fig. S2). Moreover, taking into account the expression of CD62L and CD45RO (Additional file 2: Fig. S2), the great majority of these larger CCM-derived T cells exhibited central memory (CD45R0+CD62L+) and effector memory (CD45R0+CD62L) phenotypes (Additional file 2: Fig. S2B). Of note, these lager T cell subsets were almost absent in the control group, which made any additional immune analysis impossible (Additional file 1: Fig. S1 and Fig. 1B). Among CCM patients, using the gating strategy shown in Fig. 1A, the proportion of TLR4+ (CD4+ and CD8+) T cells was found to be significantly higher in CCMSympt patients (Fig. 1B). A similar tendency was observed for TLR2+ CD4+ T cells (p = 0.0684) and TLR2+ CD8+ T cells (p = 0.0883) (Fig. 1B). Taking into account the mean fluorescence intensity (MFI), the expression of TLR4 molecules per cell was significantly higher on (CD4+ and CD8+) T cells from CCMSympt patients (Fig. 1C, D).

Fig. 1
figure 1figure 1

The frequency of cytokine-producing TLR2+ and TLR4+ T cells from CCM patients. In (B), the mean proportion of CD4+ and CD8+ T cells positive for TLR2 and TLR4, as well as (D) MFI of TLR2 and TLR4 for these cells, was determined by cytometry following representative dot-plots and histograms shown in figures A and C after acquisition of 200,000 to 300,000 events in samples obtained from asymptomatic (CCMAsympt, n = 14) and symptomatic (CCMSympt, n = 23) CCM patients. The mean percentage of these cells positive for IL-6 (E), IL-17 (F), IFN-γ (G), and IL-10 (H) was determined by flow cytometry (figure A) in the absence of stimuli (none) or 24 h after activation with Pam3Csk4 (Pam3C, 1 μg/mL) or LPS (100 ηg/mL). Data are shown as mean ± SD of seven independent experiments with 5 to 6 samples per experiment. Significance was calculated by comparing different cell culture conditions from CCMAsympt and CCMSympt groups, and the p values are shown in the figure (B and D, Ordinary ANOVA test and Turkey test; E to H, Kruskal-Wallis test and Dunn’s test).

Concerning the cell phenotypes, even without stimulation, a higher frequency of TLR2+ and TLR4+ CD4+ T cells able to produce IL-6 (Fig. 1E) and IL-17 (Fig. 1F) was detected in the CCMSympt group. Similarly, CCMSympt patients also showed a significantly higher percentage of both IL-17+CD8+ T cells, positive for TLR2 and TLR4 (Fig. 1F), and IFN-γ+ TLR4+ CD8+ T cells (Fig. 1G) than CCMAsympt patients. On the other hand, CCMAsympt group had a higher percentage of IL-10+TLR4+CD4+ T cells (Fig. 1H). From combinatorial analyses of different cytokines, we observed that the frequency of CD4+ and CD8+ T cells, expressing TLR2 or TLR4, able to simultaneously produce IL-17 and IFN-γ was significantly higher in CCMSympt than in CCMAsympt patients (Fig. 2A, B), with no difference for dual positive cells for IL-17 and IL-6 (Additional file 3: Fig. S3A) or IFN-γ and IL-6 (Additional file 3: Fig. S3B). Unfortunately, as previously demonstrated, the extremely low frequency of these T cells in samples from control group (healthy subjects) made any further analysis of the cytokine profile impossible.

Fig. 2
figure 2

An expansion of IL-17+IFN-γ+ T cells positive for TLR2 and TLR4 was observed in symptomatic CCM patients. Taking into account the representative dot-plots shown in figure (A), the mean frequency of (B) dual IL-17 and IFN-γ-secreting CD4+ and CD8+ T cells positive for TLR2 and TLR4, before and after Pam3Csk4 (Pam3C, 1 μg/mL) or LPS (100 ηg/mL) addition, was determined by cytometry after acquisition of 200,000 to 300,000 events in samples obtained from asymptomatic (CCMAsympt, n = 14) and symptomatic (CCMSympt, n = 23) CCM patients. Data are shown as mean ± SD of seven independent experiments with 5 to 6 samples per experiment. Significance was calculated by comparing different cell culture conditions from CCMAsympt and CCMSympt groups, and the p values are shown in the figure (Kruskal-Wallis test and Dunn’s test)

To determine if these TLRs are functional, the T cell subsets were reanalyzed after the addition of Pam3C and LPS. In general, CD4+ T cells were more responsive to TLR agonists than CD8+ T cells (Fig. 1E to H). Only in CD4+ T cell cultures Pam3C and LPS increased the frequency of IL-6+ cells, mainly among CCMSympt patients (Fig. 1E). Although neither Pam3C nor LPS changed the percentage of TLR+ (CD4+ and CD8+) T cells able to produce IL-17 (Fig. 1F) and IFN-γ (Fig. 1G), these TLR ligands significantly elevated the proportion of IL-17+IFNγ+ (CD4+ and CD8+) T cells in CCMAsympt and, mainly, CCMSympt patients (Fig. 2). Finally, the proportion of IL-10+ TLR4+ CD4+ T cells was only up regulated by LPS in CCMAsympt patients (Fig. 1H).

Purified CD4+ and CD8+ T cells from symptomatic CCM patients were more responsive to stimulation via TCR/CD28 complex and ligands for TLR2 and TLR4

To verify whether T cells are directly responsive to TLR2 and TLR4 ligands, T cells from CCM patients were purified and cultured for 48 h with Pam3C and LPS. As a positive control, the cells were stimulated with anti-CD3/anti-CD28-coated beads. In addition, the same analysis was performed with T cell cultures from 20 healthy adult subjects. As demonstrated in Fig. 3A, no difference concerning T cell proliferation was observed between CCM patients (asymptomatic and symptomatic) and the control group in response to either CD3/CD28 mAbs or TLR ligands. With regard to cytokine release, T cell activation via TCR/CD28 complex induced higher production of IL-6, IL-17, GM-CSF and IL-21 in cell cultures from CCMSympt patients when compared with both CCMAsympt patients and the control group (Fig. 3B). No difference was observed for TNF-α, IFN-γ and IL-10. Among TLRs, LPS was more potent than Pam3C in inducing the release of IL-6, TNF-α, IL-1β, GM-CSF, IL-17 and IL-21 by T cells in the CCMSympt group than in the CCMAsympt group (Fig. 3C). IFN-γ levels were also higher in LPS-stimulated T cell cultures from CCMSympt patients (Fig. 3C). Similar to flow cytometry result, the release of IL-10 was significantly higher in LPS-activated T cells from CCMAsympt patients (Fig. 3C). The levels of those cytokines in the supernatants from the control group were almost undetectable (data not shown).

Fig. 3
figure 3

T cells from symptomatic CCM patients were more responsive to TLR ligands and TCR/CD28 activation. T cell cultures (1 x 106/mL) from healthy subjects (Ctrl, n = 20) and CCMAsympt (n = 10) and CCMSympt (n = 10) patients were maintained in the presence of anti-CD3/anti-CD28 beads (10 μL/mL) or with ligands for TLR2 (Pam3C, 1 μg/mL) and TLR4 (LPS, 100 ηg/mL). After 48 h, the (A) T cell proliferation was determined by [3H]TdR up take, and the cytokine release after activation via TCR/CD28 (B) or TLR ligands (C) was evaluated by ELISA. Data are shown as mean ± SD of ten independent experiments with 4 samples per experiment. Significance was calculated by comparing different cell culture conditions from Ctrl, CCMAsympt and CCMSympt patients (IL-21 and GM-CSF, Kruskal-Wallis test and Dunn’s test; IL-17, IL-6, IFN-γ, IL-10, IL-1β and TNF-α, ordinary ANOVA test and Turkey test)

Elevated frequency of memory B cell subsets is observed in symptomatic CCM patients

In addition to T cells, B cells and antibodies have been found in CCM lesions [6, 27, 28]. Using CD19, CD27 and CD38, we identified naïve (CD19+CD27CD38+), memory (CD19+CD27+CD38) and memory activated (CD19+CD27+CD38+) B cells [29,30,31]. Taking into account the gate strategy shown in Fig. 4A a higher frequency of CD19+CD27+CD38, CD19+CD27+CD38+ cells (Fig. 4B), and CD19+CD27+CD38+ cells (Fig. 4C, D) was observed in CCMSympt patients as compared with control group and CCMAsympt group. All these B cells were negative for IL-10 (Fig. 4A). No difference in the frequency of B cell subsets was observed between CCMAsympt patients and control group (Fig. 4B, D).

Fig. 4
figure 4figure 4

B cell subsets in CCM patients. Following the gate strategy and representative dot-plots and histograms shown in panels (A) and (C) we determined the mean frequency of different B cell subsets in healthy subjects (Control, Ctrl, n = 20) and patients [CCMAsympt (n = 14) and CCMSympt (n = 23)] using a combination of monoclonal antibodies anti-CD19, anti-CD27, anti-CD38 and anti-IL-10. A similar analysis was performed among larger and more granular B cells in CCM patients (EG). Data are shown as mean ± SD of 5 independent experiments with 4 to 7 samples per experiment. Significance was calculated by comparing different cell culture conditions from CCMAsympt and CCMSympt groups (B and D Kruskal–Wallis and Dunn’s test; D to F, Student’s t test)

Interestingly, even showing low frequency, the percentage of CD19+CD27+CD38+ in larger and more granular cell gate was significantly higher in samples from CCMSympt than CCMAsympt patients (Fig. 4E, F). In contrast, the proportion of these cells able to produce IL-10 was significantly higher in CCMAsympt patients (Fig. 4G). Of note, these cells were negative for CD14, and very low frequency were positive for CD16 (2.78% ± 1.96%) (Additional file 1: Fig. S2A).


CCMs are vascular lesions consisting mainly of clusters of brain capillaries that are grossly dilated and present altered permeability. This predisposes patients to greater risk of hemorrhagic stroke, epilepsy and various neurological deficiencies [1]. Despite the knowledge about the genes involved in the disease, severity and outcomes of CCM depends on the activation of MEKK3-KLF2/4 pathway by external triggers [32], such as inflammatory mediators. In CCM, elevated plasma levels of IL-1β, IL-2, IFN-γ and TNF-α have been associated with disease activity [11, 33], probably by activating the MEKK3-KLF2/4 pathway [8, 9]. Interestingly, in murine model of CCM, the severity of the disease was associated with production of pro-inflammatory cytokines by endothelial cells simulated via CD14/TLR4 pathway by LPS [14]. Although the role of this PAMP in the experimental model of CCM did not depend on local immune cells, abundant innate and specific immune cells have been detected in the brain lesions in patients. Although resting T cells express very low TLR levels, these pattern receptors are strongly expressed in chronically-activated T cells associated with severity of multiple sclerosis (MS) and neuromyelitis optica spectrum disorder (NMOSD), both autoimmune diseases of the CNS [22, 24, 34, 35].

In the present study, CCMSympt patients (87% with lesional hemorrhage and 13% with seizure crisis) had a higher frequency of (CD4+ and CD8+) T lymphocytes expressing TLR4 gated in a region containing larger and more granular cells than CCMAsympt patients. This region was absent in the samples of the control group. Among the patients, the intensity of TLR4 molecule expression per (CD4 + and CD8 +) T cell was also higher in symptomatic individuals. Corresponding with their activated state, these cells were positive for some pro-inflammatory cytokines, and CCMSympt patients presented a higher proportion of IL-6+CD4+ T cells, Th17-like cells and Tc-17-like cells IL-17 cells expressing TLR2 and TLR4 than CCMAsympt patients. In addition, the symptomatic group had a higher proportion of TLR4+ Tc-1-like cells. Interestingly, clinical activity of CCM was associated with an elevated percentage of dual IL-17+ and IFN-γ+ (CD4+ and CD8+) T cells expressing TLR2 and TLR4. Furthermore, the addition of Pam3C and LPS to the cell cultures increased, mainly in CCMSympt patients, the percentage of TLR2+ and TLR4+ CD4+ T cells capable of producing IL-6 and Th17.1 cells. Preliminary analysis did not show any significant correlation between the frequency of cytokine-producing TLR+ T cell subsets and brain lesion location (data not shown). Due to financial limitations, it was not possible to evaluate the expression of other TLRs in combination with different cytokines. In line with our findings, elevated frequency of TLR+ Th17 cell subsets has been associated with MS and NMOSD [24, 26, 36,37,38].

The relationship between increased frequency of Th17 cell subsets, which classically express CCR6, and CCM clinical activity is notable, since the entry of T cells in the CNS is facilitated by the choroid plexus, a region with weak blood–brain barrier and high expression of CCL20, natural ligand of CCR6 [24, 39, 40]. In CCM areas, the local production of IL-17 and IFN-γ by Th17.1 cells would activate other local (microglia) and migrant (monocytes and B cells) immune cells, as well as endothelial cells, which increase the tissue damage. If reproduced in a larger sample size, these findings would indicate the possible involvement of autoimmune components in CCM prognosis.

Besides the expansion of pathogenic Th17 cells, autoimmune diseases are classically associated with impaired production of the anti-inflammatory cytokine IL-10 by regulatory CD4+ T cells [41,42,43,44,45]. In fact, an inverse relationship between the quantity of iron accumulated in the CCM and IL-10 was reported after a symptomatic hemorrhage [10]. Similarly, in our study, lower percentages of IL-10+TLR4+CD4+ T cells were observed in CCMSympt patients. Among the TLR ligands, LPS, but not Pam3C, enhanced both the proportion of IL-10+TLR4+CD4+ T cells and IL-10 released by purified T cells only in asymptomatic patients.

It is known that LPS responsiveness is amplified by CD14, a molecule expressed on monocyte surfaces [12, 13]. Gene polymorphisms expected to increase the expression of both membrane CD14 (mCD14) and TLR-4 have been correlated with more severe CCM disease [10, 11]. The mCD14/TLR4, when complexed to LPS, triggers intracellular signaling cascades that upregulate the production of pro-inflammatory cytokines [12, 13]. In the present study, although TLR2+ and TLR4+ T cells from CCM patients were negative for CD14, these cells responded directly to Pam3C and LPS. Here, the release of IL-6, TNF-α, IL-1β, IL-17, GM-CSF and IL-21 by purified T cells was significantly higher in CCMSympt than in CCMAsympt patients. In MS patients, the release of IL-6, IFN-γ, IL-17 and GM-CSF by Pam3C-activated CD4+ T cells was directly associated with disease activity [24]. A similar clinical correlation was observed for IL-17 levels released by Pam3C-stimulated CD8+ T cell cultures from MS patients [40]. Rajaiah et al. [46] demonstrated that while CD14 is essential for LPS-induced TLR4 activation of TRIF-mediated signaling in macrophages, this accessory molecule is not required for MyD88-mediated signaling via LPS/TLR4 complex, allowing MAPK and NF-κB activation, and TNF-α and IL-6 production. In addition, soluble CD14 (sCD14) can be involved in CCM-derived T cells responsiveness to LPS signaling in cells lacking membrane-bound CD14. Thus, the lower sCD14 levels in CCMSympt patients observed by some authors [33] may be explained by an uptake of LPS/sCD14 complex by TLR4+ T cells.

In light of the discussed above, clinical conditions associated with high circulating concentrations of LPS, as well as other PAMPs, can be triggering factors for disease activity. Interestingly, gut dysbiosis with overgrowth of GNB species has been associated with clinical activity of CCM [47,48,49]. Furthermore, endogenous TLR ligands, named danger-associated molecular patterns (DAMPs), could also contribute to the disease. Some of these DAMPs are metabolic products from the destruction of extracellular matrix by matrix metalloproteinase-2 (MMP2) produced by activated immunity cells in CCM lesions [50, 51]. Other DAMPs, such as the intracellular protein HMGB, by activating immune cells through TLR2 and TLR4 [52, 53], could also contribute to CCM pathogenesis.

Besides TLR signaling, the cytokine profile of TCR/CD28-activated T cells from CCM patients in our study was also different as an expression of clinical activity. In this context, elevated production of IL-6, IL-17 and IL-21 by purified T cells from CCMSympt individuals was observed as compared with healthy subjects and asymptomatic patients. Concerning the cytokine profile by mitogen-activated T cells, no difference between CCMasympt and control group. These results are interesting, because pathogenic GM-CSF+Th17 cell subsets, by promoting recruitment and activation of peripheral dendritic cells and monocytes, are implicated in MS pathogenesis [54,55,56], and this phenotype can also contribute to the infiltration of these phagocytes into CCM areas. Furthermore, elevated release of IL-21 and IL-6 by CCMSympt-derived T cells in response to both TLR4 ligand and TCR/CD28 signaling should contribute to local IgG production.

In addition to IgG deposits, studies by Shi et al. demonstrated the presence of well-organized clusters of CD4+ T cells, B cells, and plasma cells, which are found in CCM lesions [6, 28]. To date, it is known that somatically hypermutated IgG strictly depends on TFH cells, a newly identified CD4+ T cell subset capable of producing IL-21 and IL-6 [39], both cytokines implicated in B cell activation, generation of memory B cells and long-lived plasma cells in lymph nodes [15, 57]. The involvement of TFH cells needs to be investigated, since the activation of TFH/B cell axis could induce CCM lesions mediated by local complement activation and in situ IgG production, as described by Shi et al. [6].

With regard to B cell subsets, a higher proportion of memory (CD27+CD38) and memory activated (CD27+CD38+ and CD27+CD38++) B cells was detected in CCMSympt than in CCMAsympt patients and healthy subjects. Notably, an expansion of the CD27+CD38++ B cell subset was identified as a biomarker for relapse prediction in anti-neutrophil cytoplasmic autoantibody (ANCA)-associated vasculitis (AAV) [29], humoral autoimmune diseases involving small to medium-sized blood vessels [1]. Therefore, there is a possibility of involvement of the CD38++ B cell subset in CCM pathogenesis. Indeed, CCMSympt patients presented a higher proportion of memory B lymphocytes, among larger and granular cells, than CCMAsympt patients. In contrast, the proportion of these cells able to produce IL-10 was significantly higher in CCMAsympt patients.

Although our findings are interesting, this study has some limitations. First, this is a cross-sectional study with results based on cell cultures. A prospective study design could allow to draw conclusions about the causality between the frequency of different T and B cell subsets and the risk of new clinical events among CCM patients. Moreover, the involvement of other TLRs and their ligands needs to be investigated.


In summary, our results reveal an expansion of effector TLR2+ and, mainly, TLR4+ T cells able to produce pro-inflammatory cytokines related to Th17 and Tc-17 phenotypes in symptomatic CCM patients, in association with a decrease in the frequency of IL-10-secreting TLR4+ T cells. A similar cytokine profile was observed in TCR/CD28-activated T cells from those patients. Furthermore, expansion of memory B cell subsets was also observed in patients with clinically active CCM.

Data availability

All data generated or analyzed during this study are included in this article and its supplementary material. Further enquiries can be directed to the corresponding author.



Cerebral cavernous angioma with symptomatic hemorrhage


Cerebral cavernous malformations

CCMAsympt :

Asymptomatic cerebral cavernous malformations

CCMSympt :

Symptomatic cerebral cavernous malformations


Central Nervous System


Danger-associated molecular patterns


Expanded disability status scale


Gut dysbiosis


Granulocyte Macrophage Colony-Stimulating Factor


Gram-negative bacteria


Gram-positive bacteria


Interferon gamma




IL-1 receptor




Mitogen-activated protein kinase


Membrane CD14


Matrix by matrix metalloproteinase-2


Multiple sclerosis


Myeloid differentiation primary response protein 88


Nuclear factor-κB


Neuromyielitis optic spectrum disorders


Pathogen-associated molecular pattern


Peripheral blood mononuclear cells


Soluble CD14


Stimulation indexes


Follicular helper T


Toll-like receptor


Tumor necrosis factor


  1. Maraire JN, Awad IA. Intracranial cavernous malformations: lesion behavior and management strategies. Neurosurgery. 1995;37(4):591.

    CAS  Article  Google Scholar 

  2. Stapleton CJ, Barker FG. Cranial cavernous malformations natural history and treatment. Stroke. 2018;49(4):1029–35.

    Article  Google Scholar 

  3. Snellings DA, Hong CC, Ren AA, Lopez-Ramirez MA, Girard R, Srinath A, et al. Cerebral cavernous malformation: from mechanism to therapy. Circ Res. 2021;129(1):195–215.

    CAS  Article  Google Scholar 

  4. Caton MT, Shenoy VS. Cerebral cavernous malformations. StatPearls. StatPearls Publishing; 2021 (cited 2021 Jun 14).

  5. Zafar A, Quadri SA, Farooqui M, Ikram A, Robinson M, Hart BL, et al. Familial cerebral cavernous malformations. Stroke. 2019;50(5):1294–301.

    Article  PubMed  PubMed Central  Google Scholar 

  6. Shi C, Shenkar R, Du H, Duckworth E, Raja H, Batjer HH, et al. Immune response in human cerebral cavernous malformations. Stroke. 2009;40(5):1659–65.

    CAS  Article  Google Scholar 

  7. Crotty S. T follicular helper cell biology: a decade of discovery and diseases. Immunity. 2019;50(5):1132–48.

    CAS  Article  Google Scholar 

  8. Yang J, Lin Y, Guo Z, Cheng J, Huang J, Deng L, et al. The essential role of MEKK3 in TNF-induced NF-κB activation. Nat Immunol. 2001;2(7):620–4.

    CAS  Article  Google Scholar 

  9. Huang Q, Yang J, Lin Y, Walker C, Cheng J, Liu ZG, et al. Differential regulation of interleukin 1 receptor and toll-like receptor signaling by MEKK3. Nat Immunol. 2004;5(1):98–103.

    CAS  Article  Google Scholar 

  10. Lyne SB, Girard R, Koskimäki J, Zeineddine HA, Zhang D, Cao Y, et al. Biomarkers of cavernous angioma with symptomatic hemorrhage. JCI Insight. 2019;4(12):0–16.

  11. Girard R, Zeineddine HA, Fam MD, Mayampurath A, Cao Y, Shi C, et al. Plasma biomarkers of inflammation reflect seizures and hemorrhagic activity of cerebral cavernous malformations. Transl Stroke Res. 2018.

  12. Ciesielska A, Matyjek M, Kwiatkowska K. TLR4 and CD14 trafficking and its influence on LPS-induced pro-inflammatory signaling. Cell Mol Life Sci. 2021;78(4):1233–61.

    CAS  Article  PubMed  Google Scholar 

  13. Zanoni I, Otsuni R, Marek LR, Barresi S, Barbalat R, Barton GM, et al. CD14 controls the LPS-induced endocytosis of Toll-like Receptor 4. Cell. 2011;147(4):868–80.

    CAS  Article  Google Scholar 

  14. Tang AT, Choi JP, Kotzin JJ, Yang Y, Hong CC, Hobson N, et al. Endothelial TLR4 and the microbiome drive cerebral cavernous malformations. Nature. 2017;545(7654):305–10.

    CAS  Article  Google Scholar 

  15. Vinuesa CG, Linterman MA, Yu D, MacLennan ICM. Follicular helper T cells. Annu Rev Immunol. 2016;34(1):335–68.

    CAS  Article  Google Scholar 

  16. Couture A, Garnier A, Docagne F, Boyer O, Vivien D, Le-Mauff B, et al. HLA-Class II artificial antigen presenting cells in CD4+ T cell-based immunotherapy. Front Immunol. 2019;10:1–11.

    Article  Google Scholar 

  17. Jin B, Sun T, Yu XH, Yang YX, Yeo AET. The effects of TLR activation on T-cell development and differentiation. Clin Dev Immunol. 2012; 2012(Figure 1).

  18. Dobrzanski MJ, Reome JB, Hollenbaugh JA, Dutton RW. Tc1 and Tc2 effector cell therapy elicit long-term tumor immunity by contrasting mechanisms that result in complementary endogenous type 1 antitumor responses. J Immunol. 2004;172(3):1380–90.

    CAS  Article  Google Scholar 

  19. Liang Y, Pan HF, Ye DQ. Tc17 cells in immunity and systemic autoimmunity. Int Rev Immunol. 2015;34(4):318–31.

    CAS  Article  Google Scholar 

  20. Cosmi L, Maggi L, Santarlasci V, Liotta F, Annunziato F. T helper cells plasticity in inflammation. Cytometry Part A. 2014.

  21. Frank PG, Lisanti MP. ICAM-1: role in inflammation and in the regulation of vascular permeability. Am J Physiol Heart Circ Physiol. 2008;295(3):H926–7.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  22. Barros PO, Dias ASO, Kasahara TM, Ornelas AMM, Aguiar RS, Leon SA, et al. Expansion of IL-6+ Th17-like cells expressing TLRs correlates with microbial translocation and neurological disabilities in NMOSD patients. J Neuroimmunol. 2017;307:82–90.

    CAS  Article  PubMed  Google Scholar 

  23. Dias ASO, Sacramento PM, Lopes LM, Sales MC, Castro C, Araújo ACRA, et al. TLR-2 and TLR-4 agonists favor expansion of CD4+ T cell subsets implicated in the severity of neuromyelitis optica spectrum disorders. Multiple Sclerosis Related Disord. 2019;34:66–76.

    Article  Google Scholar 

  24. Ferreira TB, Hygino J, Wing AC, Kasahara TM, Sacramento PM, Camargo S, et al. Different interleukin-17-secreting Toll-like receptor + T-cell subsets are associated with disease activity in multiple sclerosis. Immunology. 2018;154(2):239–52.

    CAS  Article  Google Scholar 

  25. Miranda-Hernandez S, Baxter AG. Role of toll-like receptors in multiple sclerosis. Am J Clin Exp Immunol. 2013;2(1):75–93.

    PubMed  PubMed Central  Google Scholar 

  26. Voo KS, Bover L, Harline ML, Weng J, Sugimoto N, Liu Y-J. Targeting of Toll-like receptors inhibits CD4+ regulatory T cell function and activates lymphocytes in human PBMCs. J Immunol. 2014;193(2):627–34.

    CAS  Article  Google Scholar 

  27. Shi C, Shenkar R, Zeineddine HA, Girard R, Fam MD, Austin C, et al. B-cell depletion reduces the maturation of cerebral cavernous malformations in murine models. J Neuroimmune Pharmacol. 2016;11(2):369–77.

    Article  PubMed  PubMed Central  Google Scholar 

  28. Shi C, Shenkar R, Kinloch A, Henderson SG, Shaaya M, Chong AS, et al. Immune complex formation and in situ B-cell clonal expansion in human cerebral cavernous malformations. J Neuroimmunol. 2014;272:67–75.

    CAS  Article  PubMed  Google Scholar 

  29. von Borstel A, Land J, Abdulahad WH, Rutgers A, Stegeman CA, Diepstra A, et al. CD27+CD38hi B cell frequency during remission predicts relapsing disease in granulomatosis with polyangiitis patients. Front Immunol. 2019;10:1–10.

    Article  Google Scholar 

  30. Bergantini L, d’Alessandro M, Cameli P, Vietri L, Vagaggini C, Perrone A, et al. Effects of rituximab therapy on B cell differentiation and depletion. Clin Rheumatol. 2020;39(5):1415–21.

    CAS  Article  Google Scholar 

  31. Clavarino G, Delouche N, Vettier C, Laurin D, Pernollet M, Raskovalova T, et al. Novel strategy for phenotypic characterization of Human B lymphocytes from precursors to effector cells by flow cytometry. PLoS ONE. 2016;11(9):1–16.

    Article  Google Scholar 

  32. Stockton RA, Shenkar R, Awad IA, Ginsberg MH. Cerebral cavernous malformations proteins inhibit Rho kinase to stabilize vascular integrity. J Exp Med. 2010;207(4):881–96.

    CAS  Article  Google Scholar 

  33. Girard R, Zeineddine HA, Koskimäki J, Fam MD, Cao Y, Shi C, et al. Plasma biomarkers of inflammation and angiogenesis predict cerebral cavernous malformation symptomatic hemorrhage or lesional growth short communication. Circ Res. 2018;122(12):1716–21.

    CAS  Article  Google Scholar 

  34. Cantorna MT, Waddell A. The vitamin D receptor turns off chronically activated T cells. Ann N Y Acad Sci. 2014;1317(1):70–5.

    CAS  Article  Google Scholar 

  35. Cope AP. Studies of T-cell activation in chronic inflammation. Arthritis Res. 2002;4:S197-211.

    Article  Google Scholar 

  36. van Langelaar J, van der Vries VDRM, Janssen M, Wierenga-Wolf AF, Spilt IM, Siepman TA, et al. T helper 17.1 cells associate with multiple sclerosis disease activity: perspectives for early intervention. Brain. 2018;141:1334–49.

    Article  Google Scholar 

  37. Sales MC, Kasahara TM, Sacramento PM, Rossi ÁD, Cafasso MOSD, Oyamada HAA, et al. Selective serotonin reuptake inhibitor attenuates the hyperresponsiveness of TLR2+ and TLR4+ Th17/Tc17-like cells in multiple sclerosis patients with major depression. Immunology. 2021;162:290–305.

    CAS  Article  Google Scholar 

  38. Wing AC, Hygino J, Ferreira TB, Kasahara TM, Barros PO, Sacramento PM, et al. Interleukin-17- and interleukin-22-secreting myelin-specific CD4 + T cells resistant to corticoids are related with active brain lesions in multiple sclerosis patients. Immunology. 2016;147(2):212–20.

    CAS  Article  PubMed  Google Scholar 

  39. Teixeira B, Bittencourt VCB, Ferreira TB, Kasahara TM, Barros PO, Alvarenga R, et al. Low sensitivity to glucocorticoid inhibition of in vitro Th17-related cytokine production in multiple sclerosis patients is related to elevated plasma lipopolysaccharide levels. Clin Immunol. 2013;148(2):209–18.

    CAS  Article  PubMed  Google Scholar 

  40. Mony JT, Khorooshi R, Owens T. Chemokine receptor expression by inflammatory T cells in EAE. Front Cell Neurosci. 2014;8:1–9.

    Article  Google Scholar 

  41. Dominguez-Villar M, Hafler DA. Regulatory T cells in autoimmune disease. Nat Immunol. 2018;19(7):665–73.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  42. Zhang X, Olsen N, Zheng SG. The progress and prospect of regulatory T cells in autoimmune diseases. J Autoimmun. 2020;111: 102461.

    CAS  Article  PubMed  Google Scholar 

  43. Danikowski KM, Jayaraman S, Prabhakar BS. Regulatory T cells in multiple sclerosis and myasthenia gravis. J Neuroinflamm. 2017;14(1):117.

    CAS  Article  Google Scholar 

  44. Tian G, Li JL, Wang DG, Zhou D. Targeting IL-10 in auto-immune diseases. Cell Biochem Biophys. 2014;70(1):37–49.

    CAS  Article  Google Scholar 

  45. Fujio K, Okamura T, Yamamoto K. The family of IL-10-secreting CD4 + T cells. Adv Immunol. 2010;105:99–130.

    CAS  Article  PubMed  Google Scholar 

  46. Rajaiah R, Perkins DJ, Ireland DDC, Vogel SN, Kagan JC. CD14 dependence of TLR4 endocytosis and TRIF signaling displays ligand specificity and is dissociable in endotoxin tolerance. Proc Natl Acad Sci USA. 2015;112(27):8391–6.

    CAS  Article  Google Scholar 

  47. Awad IA, Polster SP. Cavernous angiomas: deconstructing a neurosurgical disease. J Neurosurg. 2019;131(1):1–13.

    CAS  Article  Google Scholar 

  48. Tang AT, Sullivan KR, Hong CC, Goddard LM, Mahadevan A, Ren A, et al. Distinct cellular roles for PDCD10 define a gut-brain axis in cerebral cavernous malformation. Sci Transl Med. 2019.

    Article  PubMed  PubMed Central  Google Scholar 

  49. Bibbò S, Dore MP, Cammarota G. Response to: Comment on “gut microbiota as a driver of inflammation in nonalcoholic fatty liver disease”. Mediators of Inflammation. 2018; 2018.

  50. Frevert CW, Felgenhauer J, Wygrecka M, Nastase MV, Schaefer L. Danger-associated molecular patterns derived from the extracellular matrix provide temporal control of innate immunity. J Histochem Cytochem. 2018;66(4):213–27.

    CAS  Article  Google Scholar 

  51. Roh JS, Sohn DH. Origin and list of DAMPS. Immune Netw. 2018;18(4):1–14.

    Article  Google Scholar 

  52. Zindel J, Kubes P. DAMPs, PAMPs, and LAMPs in immunity and sterile inflammation. Annu Rev Pathol. 2020;15(1):493–518.

    CAS  Article  Google Scholar 

  53. Yu M, Wang H, Ding A, Golenbock DT, Latz E, Czura CJ, et al. HMGB1 signals through toll-like receptor (TLR) 4 and TLR2. Shock. 2006;26(2):174–9.

    CAS  Article  Google Scholar 

  54. Restorick SM, Durant L, Kalra S, Hassan-Smith G, Rathbone E, Douglas MR, et al. CCR6+ Th cells in the cerebrospinal fluid of persons with multiple sclerosis are dominated by pathogenic non-classic Th1 cells and GM-CSF-only-secreting Th cells. Brain Behav Immun. 2017;64:71–9.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  55. Aram J, Francis A, Tanasescu R, Constantinescu CS. Granulocyte-macrophage colony-stimulating factor as a therapeutic target in multiple sclerosis. Neurol Therapy. 2019;8(1):45–57.

    Article  Google Scholar 

  56. Rasouli J, Ciric B, Imitola J, Gonnella P, Hwang D, Mahajan K, et al. Expression of GM-CSF in T cells is increased in multiple sclerosis and suppressed by IFN-β Therapy. J Immunol. 2015;194(11):5085–93.

    CAS  Article  Google Scholar 

  57. Schmitt N, Bentebibel SE, Ueno H. Phenotype and functions of memory Tfh cells in human blood. Trends Immunol. 2014;35(9):436–42.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

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This work was supported by the funds provided by the Brazilian Parliamentary Rare Diseases Initiative.

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Authors and Affiliations



JPBMS, SVAL and GFG contributed by discussing hypothesis generation, patient monitoring and sample collection throughout the CCM cohort of the University Hospitals of the Federal University of Rio de Janeiro and Federal State University of Rio de Janeiro. CAMB and JM designed the study and wrote the paper. CC, HAAO, MOSDC, JH, CM, PMS and LML performed the experiments. CAMB and CC analyzed the data. Brazil Cavernous Alliance contributed with vital reagents. All authors participated in critical revision of the manuscript, provided important intellectual input and approved the final version. All authors read and approved the final manuscript.

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Correspondence to Cleonice A. M. Bento.

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This study was approved by the Ethics Committee for Research on Human Subjects at the Federal University of the State of Rio de Janeiro (UNIRIO) (CAAE:69409617.9.0000.5258) and blood samples were collected only after written informed consent was obtained from each individual.

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Supplementary Information

Additional file 1: Fig. S1.

Percentage of TLR4+ T cells in healthy subjects (n = 20) and asymptomatic (n = 14) and symptomatic (n = 23) CCM patients. In B, the mean percentage of TLR-4+ (CD4+ an CD8+) T cells from each experimental group was determined and significance calculated by comparing different experimental groups (Kruskal–Wallis test and Dunn’s test).

Additional file 2: Fig. S2.

Phenotypic characterization of T cells, expressing TLR, and B cells gated on larger and more granular cells from CCM patients. In (A), the gating strategy and identification of different larger and more granular lymphocytes according to the expression of CD3, CD19, CD14, CD16 and CD45RO markers. In (B), the mean percentage of naïve (CDR5ROCD62L+), central memory (CM, CDR5RO+CD62L+), effector memory (EM, CDR5RO+CD62L) and terminally differentiated effector memory (TEMRA, CD45ROCD62L) T cells from CCM patients was determined and significance calculated by comparing the proportion of different T cell phenotypes according CD45RO and CD62L expression (Kruskal–Wallis test and Dunn’s test).

Additional file 3: Fig. S3.

Frequency of IL-17+IL-6+ and IL-6+IFN-γ+ T cells expressing TLR2 and TLR4 in CCM patients. The mean frequency of dual (A) IL-17 and IL-6- or (B) IL-17 and IFN-γ-secreting (CD4+ and CD8+) T cells positive for TLR2 and TLR4 from asymptomatic (CCMAsympt, n = 14) and symptomatic (CCMSympt, n = 23) patients was determined before and after Pam3Csk4 (Pam3C, 1 μg/mL) or LPS (100 ηg/mL) addition. Data are shown as mean ± SD of seven independent experiments with 5 to 6 samples per experiment. Significance was calculated by comparing different cell culture conditions from CCMAsympt and CCMSympt groups, and the p values are > 0.05 (Kruskal–Wallis test and Dunn’s test).

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Castro, C., Oyamada, H.A.A., Cafasso, M.O.S.D. et al. Elevated proportion of TLR2- and TLR4-expressing Th17-like cells and activated memory B cells was associated with clinical activity of cerebral cavernous malformations. J Neuroinflammation 19, 28 (2022).

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  • Cerebral cavernous malformations
  • T cells
  • Th17 cells
  • TLR
  • Cytokines
  • B cells
  • LPS