SSc skin contains increased numbers of activated cytotoxic T and NK cells with a cytolytic proinflammatory and profibrotic signature

T and NK cell subsets may upregulate costimulatory receptors to direct the autoimmune inflammatory process in SSc. To gain a comprehensive profiling of skin infiltrating lymphocytes, we analysed T and NK cell clusters (n=5061 cells) from a scRNAseq dataset of affected skin of 97 SSc patients compared with healthy skin from 56 individuals, as part of a larger dataset that was published recently (GSE195452)10 (online supplemental figure 1). To enhance confidence, we comparatively analysed another single-cell RNA transcriptome dataset containing 2126 cells from 9 healthy and 12 SSc skin biopsies (GSE138669)11 (online supplemental figure 2).

First, we analysed T cells and NK cells in skin single-cell datasets based on differential gene expression of known lineage-specific genes (GSE195452, GSE138669). Among the transcriptionally distinct cell subtypes that were detected (online supplemental figures 1A and 2A), the following three were significantly expanded (q<0.05 for all comparisons) in SSc compared with healthy skin in both datasets: proliferating T cells, CD8⁺ cytotoxic T cells and NK cells (figure 1A,B). We verified the presence of these T and NK cell subsets at the protein level in SSc-affected skin in an additional cohort of 24 SSc patients (figure 1C). In addition, increased infiltration of cytotoxic CD8⁺ T cells and CD56⁺ NK cells was further apparent in biopsies from the affected compared with matched non-affected skin in 71% and 83% of SSc patients, respectively (n=24, p=0.06 and p<0.001, respectively) (figure 1D,E). In the affected SSc skin, cytotoxic T cells and NK cells were primarily present in perivascular areas while a smaller amount of these cells was infiltrated around blood vessels of the non-affected skin (figure 1D, online supplemental figure 4C).

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Figure 1

Increased frequency of profibrotic cytotoxic T cells and NK cells in SSc skin. (A) Frequencies of T cell and NK cell clusters in the skin of (n=56) healthy donors (HD) compared with (n=97) patients with SSc (GSE195452). (B) Frequencies of T cell and NK cell clusters in the skin of (n=9) HD compared with (n=12) patients with SSc (GSE138669). For both panels (A, B), values are represented as variation in cell counts (in %) and statistics were performed with Wilcox-Test, corrected for multiple comparisons. Only the adjusted p values (q) of the statistically significant comparisons are shown, *q<0.05, **q<0.01. (C) Representative multicolor immunofluorescence composite image of T helper CD3⁺CD8⁻ (red), cytotoxic CD8⁺ (cyan), regulatory FOXP3⁺ (green) T cells and CD56⁺CD3⁻ (yellow) NK cells in SSc-affected skin. (D) Immunofluorescence composite images of infiltrated cytotoxic CD8⁺ (cyan) T cells and CD56⁺CD3⁻ (yellow) NK cells of the non-affected versus the affected skin from a representative SSc patient with early diffuse cutaneous disease. (E) Percentages (%) of cytotoxic T (CD3⁺CD8⁺) and NK cells (CD56⁺CD3⁻) in matched non-affected versus affected SSc skin (n=24 SSc patients). Values are represented as % of CD3⁺CD8⁺ or CD56⁺CD3⁻ cells compared with all cells (DAPI⁺) present in each biopsy (excluding the rich in keratinocytes epidermis layer). Statistics were performed with non-parametric Wilconxon test, ***p<0.001. (F) (left) Gene set enrichment analysis of skin T cell and NK cell clusters with Wiki pathways as reference dataset. Examples of top pathways (p<0.001) represented by NK and CTL clusters are shown. Statistics were performed with Kolmogorov-Smirnov (KS) test. (Right) Comparison of the enrichment scores of the ‘’Overview of proinflammatory and profibrotic mediators’' (q=0.025) and ‘'Lung fibrosis’’ (q=0.0002) pathways in HD (green) vs SSc (red) skin T and NK cell clusters (GSE195452). (G) (Left) UMAP displaying 5 transcriptionally different CD8⁺ T cell clusters in skin of (n=56) HD and (n=97) SSc, n=977 cells. Based on the top differentially expressed genes, clusters were annotated as naïve (T naive), Granzyme K⁺ (GZMK⁺), Granzyme B⁺ (GZMB⁺), exhausted (Texh) and proliferating (Tprolif). (right) Cell frequency of CD8⁺ T cell clusters between HD and SSc. (H) Percentage of Granzyme B (GZMB) expressing CD8⁺ T cells in peripheral blood of (n=15) HD and (n=30) SSc. Values are represented as percentage of total live peripheral blood mononuclear cells, *p<0.05. CTLs, cytotoxic T cells; BV, blood vessel; HF, hair follicle; NK, natural killer; SSc, systemic sclerosis; Thprm, hypofunctional tissue resident T cells; Tncm, naïve/central memory; Tprolif, proliferating T cells; Tqcm, quiescent tissue- resident T cells; Tregs, regulatory T cells; Trm, tissue-resident memory T cells.

Next, we analysed the potential function of these enriched cell populations in SSc skin. For this, we used gene set enrichment analyses based on each cluster’'s differentially expressed genes with Wiki pathways as reference dataset. Both the skin cytotoxic T and NK cell clusters from each sc-dataset were not only associated with cell cytolytic pathways, but were also the only clusters from SSc skin that were specifically enriched for gene sets related to lung fibrosis, proinflammatory and profibrotic manifestations relative to healthy skin (figure 1F, online supplemental figure 2C). These pathways included profibrotic genes such as TGFB1, XCL1, OSM, CCL4, IL4, IL17, FGF and PDGF (for a complete overview see online supplemental figure 3). This indicates that cytotoxic cells are not only involved in cytotoxicity but also in directing profibrotic pathophysiological processes.

In recent studies in chronic inflammatory conditions, CD8⁺ T cells were shown to mainly exert a cytokine-mediated function instead of their conventional cytotoxic effects with an important role of granzyme K.12 Therefore, we performed a focused analysis of CD8⁺ T cells. In skin, at the sc-RNAseq level, the following CD8⁺ subclusters were formed: naïve, proliferating, skin resident exhausted like, granzyme K (GZMK⁺) and granzyme B (GZMB⁺) positive effector cells. Of these, only the subset of CD8 effector GZMB⁺ cells were significantly enriched in SSc skin (figure 1G, online supplemental figure 1D). Flow cytometry analysis in blood also showed increased (twofold) presence of CD8⁺GZMB⁺ cells in SSc compared with healthy donors (figure 1H).

Expanded CD8⁺ T and NK cells in the affected skin and lungs of SSc patients are characterised by upregulation of the CD7 costimulatory molecule

The activity of cytotoxic T cells and NK cells is closely regulated by an interplay between activating and inhibitory cell surface receptors. In chronic infection and malignancies, T and NK cell cytotoxic functions are restricted by inhibitory receptors.13–15 Therefore, we compared expression of known T and NK cell activating and inhibitory receptors between immune cells of healthy and SSc skin. Of the inhibitory receptors, LAG3 was expressed in a proportion of CD8⁺GZMB⁺ T cells in SSc skin. The expression of TIGIT, CTLA4 and HAVCR2 (TIM-3) did not show any significant difference between healthy and SSc skin while PDCD1 (PD-1) was only expressed in a few naïve/central memory CD8⁺ T cells together with FOXP3 (online supplemental figure 1E). Of the activating receptors, CD69 and CD7 were upregulated in CD8⁺GZMB⁺ T cells while SSc NK cells exhibited elevated expression of CD7, TNFRSF9 (CD137) and CD28. In the cluster of proliferating SSc T cells, CD40LG was downregulated and CD28 expression was decreased in SSc versus healthy skin (figure 2A). Of these, CD7 was expressed by almost all the cells in these clusters (online supplemental figure 4D) and also showed the strongest upregulation in patients compared with controls (q<0.001) (figure 2A,B). In a further attempt to identify differences in cytotoxic T and NK cell activation between healthy and SSc individuals, we used an alternative unbiased approach based on the FindConservedMarker function implemented in Seurat (to find features that are conserved between the groups, ie, healthy donors and SSc). This approach confirmed enrichment of cytotoxic genes and CD7 in cytotoxic T cells and NK cells of SSc patients compared with healthy controls. No other activating or inhibitory receptors were enriched in SSc in this analysis (figure 2C). These observations suggest that CD7 costimulation may be involved in SSc skin T and NK cell activation.

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Figure 2

CD7 upregulation associates with activation of cytotoxic T and NK cells in SSc-affected skin and lungs. (A) Two-dimensional dot plots comparing the gene expression of selected activating and inhibitory costimulatory receptors in Tprolif, CD8⁺GZMB⁺ and NK clusters between HD and SSc (circle size shows the percentage of cells expressing each gene and colour intensity depicts average expression while numbers indicate average of normalised counts), *p<0.05 and **p<0.01. (B) (Top) UMAPs representing positive (red) and negative (grey) gene expression of CD7 among CD8⁺ T cells (left) and CD56⁺ NK cells (right). (Bottom) Intensity of CD7 normalised gene expression between HD and SSc among CD8⁺ T cells (left) and CD56⁺ NK cells (right). (C) Scatter plot with gene expression values highlighting genes that are specifically enriched in skin T and NK cells of patients with SSc compared with HD. (D) Representative photos of CD7 immunohistochemistry (IHC) staining of the affected and non-affected skin biopsies from an SSc patient, accompanied by quantification of CD7 IHC scores (n=20). Non-parametric sign test, *p<0.05. (E) Immunofluorescence microscopy showing coexpression of CD7 with CD8⁺ T and CD56⁺ NK cells in early dSSc skin. A representative experiment is depicted in scale of 100 µm. (F) (Left) UMAP displaying T and NK cells from control (healthy) (n=6) and SSc (n=7) lung tissues from patients with interstitial lung disease (GSE128169). (Middle) Density plots showing gene expression density of CD7, NCAM1 (CD56), CD4 and CD8A. (Right) CD7 gene expression counts (normalised) between control and SSc lung T and NK cells (each dot represents the average CD7 expression per donor). SSc, systemic sclerosis.

To validate these results at the protein level, we performed CD7 and CD3 immunohistochemistry in SSc skin tissue. The total amount of CD3⁺ T cells was higher even though statistically non-significant in the affected SSc skin (mean number of CD3⁺ T cells: 15.8 affected vs 6.1 in non-affected) (online supplemental figure 4A,B). Strikingly, an increased infiltration of CD7⁺ cells was specifically found in the perivascular areas (online supplemental figure 4C) of affected compared with the non-affected SSc skin (figure 2D). Furthermore, in SSc skin, CD7 was found to be coexpressed with CD8 and CD56 positive cells, while no expression on CD3⁺CD8⁻ cells could be observed (figure 2E).

Recently, an increased presence of tissue-resident cytotoxic T and NK cells was also described in SSc lungs.16 Thus, we next evaluated CD7 expression in SSc lung tissue compared with healthy. In accordance with our data in skin, CD7 was selectively expressed in lung cytotoxic T cells and NK cells and its expression in SSc CD8⁺ T cells and CD56⁺ NK cells was significantly higher (twofold increase) compared to healthy counterparts (figure 2F). In conclusion, CD7 is a costimulatory receptor that is significantly upregulated in disease-related cytotoxic immune cell populations in both the affected skin and lungs of patients with SSc.

CD7 costimulation is involved in T and NK cell cytotoxic and profibrotic processes

CD7 is upregulated after TCR ligation and activated by its ligand, SECTM1.17 SECTM1 is a transmembrane protein produced by thymic epithelial cells and fibroblasts and induced by IFN-γ in professional antigen-presenting cells. CD7 activation by SECTM1 has been shown to augment CD4⁺ and CD8⁺ T cell effector functions.18 To gain insight on the function of CD7 in SSc, we analysed expression of SECTM1 in skin stromal and immune cells. In our dataset, SECTM1 as expected was primarily detected in skin myeloid cells including monocytes, macrophages and dendritic cells. Furthermore, SECTM1 was also expressed by cells in the fibroblast cluster characterised by increased expression of Prostaglandin D Synthase (PTGDS) (figure 3A). Interestingly, it was previously reported that this fibroblast subtype is marked by high expression of MHC class I genes compared with other skin fibroblast subsets, suggesting that the SECTM1-CD7 axis may be important in T and NK cell activation (online supplemental figure 5A). Notably, T cell and NK cell CD7 expression was positively correlated with IFNG, while expression of its receptor (IFNGR1) positively correlated with SECTM1 in fibroblasts and antigen presenting cells (online supplemental figure 5B,C). This suggests an IFN-γ-driven SECTM1-CD7 axis in SSc skin.

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Figure 3

CD7 costimulation plays an essential role in T and NK cell cytotoxic and profibrotic manifestations. (A) SECTM1 log normalised gene expression among skin immune and stromal cell subsets (GSE195452). Annotation of the depicted cell clusters were retrieved from Gur et al.10 (B) Subgroup analysis of CD7 normalised gene expression among healthy individuals (HD), and systemic sclerosis (SSc) patients with early versus late limited cutaneous SSc (lSSc) or diffuse cutaneous (dSSc) disease. Early disease was defined as ≤3 years from initial diagnosis. One-way ANOVA with Tukey’s multiple comparisons test, *p<0.05, ***p<0.001. (C) (Left) Scatter plot showing correlation of CD7 normalised gene expression with skin score. Each circle represents a single SSc patient. Spearman’s r=0.34, p=0.07. (Right) Normalised CD7 gene expression between SSc patients with low versus high skin scores. The distinction between low and high skin score was as described previously.10 (D) Normalised CD7 gene expression between SSc patients who were treatment naïve or treated with immunosuppressive medication and between SSc patients with or without the presence of interstitial lung disease (ILD). (E) Percentage of CD8⁺CD7⁺ and CD8⁺CD7⁻ T cells in peripheral blood of (n=15) HD and (n=30) SSc. Values are represented as percentage of total CD3⁺ T cells, *p<0.05. (F) Expression (mean fluorescence intensity, MFI) of Granzyme B (GZMB) and percentage of IL-4⁺/IL-13⁺ cells between HDs and SSc CD8⁺CD7⁺ T cells. Expression levels of GZMB are presented as MFI and values of IL-4⁺/IL-13⁺ cells are represented as percentage of positive cells among the CD8⁺CD7⁺ T cell compartment. Student’s t-test, *p<0.05. (G) Cytolytic activity of T and NK cells in a coculture with K562 target cells was quantified by measuring lactate dehydrogenase (LDH) release of the target cells. T cells and NK cells were stimulated with anti-CD3/CD28 and IL-2/IL-15, respectively, and anti-CD7 was added to block CD7 costimulation. Unstim refers to control cells that were not stimulated. Statistical comparisons between groups were performed with ordinary one-way ANOVA with Tukey’s multiple comparisons test *p<0.05, **p<0.01, ***p<0.001. (H) Pairwise correlation plots between CD7 and XCL1, TGB1, OSM, MMP9 gene expression within the NK or cytotoxic T cell (CTLs) clusters in SSc-affected skin (GSE195452). ANOVA, analysis of variance; SSc, systemic sclerosis.

From a clinical perspective, SSc is a heterogeneous disease with various disease subtypes and phases. Thus, we next analysed CD7 gene expression in subgrouping of SSc patients with limited (lSSc) versus diffuse (dSSc) cutaneous and early (≤3 years from first non-Raynaud symptom) versus late disease. We found that CD7 was significantly upregulated in early diffuse SSc compared with late disease (figure 3B) and CD7 expression was further associated with patients exhibiting increased skin score (p=0.03) (figure 3C). CD7 skin expression was not associated with the presence of interstitial lung disease. Furthermore, CD7 expression was similar between treatment naïve and patients who were receiving immunosuppressive medication, suggesting that currently used therapeutic approaches do not seem to directly target this activation axis (figure 3D).

To further explore the function of CD7⁺ T cells, we analysed the response to activation of cells purified from blood. In SSc blood, a larger fraction of CD8⁺CD7⁺ cells were detected compared with healthy individuals (18% of total CD3⁺ cells in SSc vs 12% in HD) (figure 3E). The CD7⁺CD8⁺ T cells from SSc patients on short (t=4 hours) stimulation with phorbol myristate acetate and ionomycin produced significantly more granzyme B (MFI: 40 000 in SSc vs 34 000 in HD). In addition, SSc CD8⁺CD7⁺ T cells were also characterised by increased coexpression of the profibrotic cytokines IL-4 and IL-13 (among CD8⁺ T cells: 2.5% IL-13⁺ and 40% IL-4⁺) compared with CD8⁺CD7⁺ cells of healthy controls (among CD8⁺ T cells: 1% IL-13⁺ and 30% IL-4⁺) (figure 3F). Taken together, these data indicate that CD8⁺ T and NK cells that exhibit cytotoxic and profibrotic properties in SSc, are characterised by increased CD7 expression.

To test the involvement of CD7 in T and NK cell cytotoxicity, we cocultured healthy peripheral blood mononuclear cells (PBMCs) (n=6) with K562 cancer cells and evaluated T and NK cell cytolytic activity by measuring the release of lactate dehydrogenase from the damaged target cells. Interestingly, while blockage of the CD7 receptor did not affect the cell viability of T and NK cells, it was accompanied by significant reduction in their cytolytic capacity towards K562 cells (figure 3G). This observation suggests that CD7 costimulation is important for an efficient cytotoxic response.

In addition, we observed above that SSc skin cytotoxic T and NK cells showed disease-related enrichment of pathways associated with lung fibrosis and proinflammatory/profibrotic manifestations. To explore the potential involvement of CD7 in the observed profibrotic manifestations of the cytotoxic skin cells, we obtained and merged the gene lists associated with those pathways and performed pairwise correlations with CD7 (online supplemental figure 3). Notably, CD7 gene expression in SSc-affected skin was positively correlated with expression of profibrotic mediators such as XCL1 19 20 and CCL3 21 22 in cytotoxic lymphocytes (CTLs) and TGFB1 23 24 and OSM 25 26 in NK cells (figure 3H). From these observations, it is suggested that CD7 costimulation regulates both T and NK cell mediated cytotoxicity and fibrosis.

In vitro elimination of the expanded and activated CD7⁺ T and NK cell subsets by targeted immunotoxin treatment halts fibroblast contraction

The selective upregulation of CD7 expression in cytotoxic T and NK cells in SSc skin can serve as target for therapeutic modulation but also selective depletion of these cells. For this, we used a combination of anti-CD3/CD7 immunotoxins (CD3/CD7-IT) developed to target alloreactive activated T cells and NK cells in graft versus host disease (GvHD).27 In cultured PBMCs isolated from patients’ blood, a significant killing efficacy (>85% cells eliminated) of CD3/CD7-IT was only observed towards the activated T cells and NK cells (figure 4A). The combination of CD3 and CD7 immunotoxins had an additive effect on the killing efficacy towards T cells, while NK cells (CD3-CD56+CD7+) as expected were predominantly targeted by the CD7-IT (figure 4B). Of note, treatment with CD3/CD7-IT also effectively depleted the potentially pathogenic CD8⁺GZMB⁺ T cells and CD56⁺GZMB⁺ NK cells (figure 4C). IL-2 production was ninefold decreased on treatment (online supplemental figure 6A), supporting that anti-CD3/CD7-IT treatment selectively depleted the activated T cells and NK cells. The surviving CD8⁺ T cells in the CD3/CD7-IT treated condition exhibited a clear alteration in their memory/maturation status: decreased CD8 effector and increased memory and naïve phenotype, showing killing specificity towards effector cells (online supplemental figure 6B). Additionally, on post-treatment stimulation with PHA, the CD8+T cells that survived treatment showed diminished cell proliferation (decreased % CD8⁺Ki-67⁺ cells) and production of cytotoxic (GZMB) and profibrotic molecules (IL-4) compared with their non-treated counterparts (online supplemental figure 6C). Importantly, treatment with anti-CD3/CD7-IT had no effect on the number nor the cell viability of CD19⁺ B cells and CD14⁺ M2 monocytes/macrophages (online supplemental figure 6D,E). Next, we used ex vivo whole skin cultures and showed that on treatment with anti-CD3/CD7-IT, both numbers of CD8⁺ T cells and CD56⁺ NK cells were significantly reduced compared with the untreated condition (figure 4D).

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Figure 4

Targeted immunotoxin mediated depletion of activated CD7⁺ T cells and CD7⁺ NK cells prevents fibroblast contraction and decreases myofibroblast phenotype (A) Flow cytometric quantification of CD3/CD7-IT-induced cell death exhibiting absolute cell counts (cells/µl) of CD2⁺ T and CD56⁺ NK cells in PBMCs isolated from (n=5) SSc patients. (B) Percentage of normalised cell viability of CD3⁺ T and CD56⁺ NK cells isolated from SSc (n=3) PBMCs. (C) Flow cytometric quantification of CD3/CD7-IT-induced cell death illustrating absolute cell counts (cells/µl) of CD8⁺GZMB⁺ T and CD56⁺GZMB⁺ NK cells in PBMCs isolated from (n=5) SSc patients. (D) Flow cytometric quantification of CD3/CD7-IT-induced cell death towards CD8⁺ T and CD56⁺ NK cells in ex vivo skin explants (n=4). Paired t-test, *p<0.05, **p<0.01.(E) Schematic representation of our in vitro hydrogel collagen contraction assay in the developed three-dimensional (3D) model with cocultured primary skin fibroblasts and PBMCs. The level of contraction was quantified compared with no-cells control and plotted graphically on the right (n=3). Bars are mean±SD. An image of a representative experiment is depicted on the bottom of this panel. (F) The percentage of proapoptotic cytotoxic T (CD8⁺7-AAD⁻Annexin V⁺) and NK (CD56⁺7-AAD⁻Annexin V⁺) cells in the depicted conditions was measured with flow cytometry of the enzymatically digested collagen plugs (n=5). (G) IgG or CD3.CD7-IT treated PBMCS were cocultured with primary dermal fibroblasts in the developed 3D hydrogel collagen coculture model and fibroblasts were analysed for expression of genes reflective of a myofibroblast phenotype. Values represent relative gene expression (−ΔCt) as measured with qPCR. GAPDH and RPS27A were used as reference genes. Data represent mean ± SEM. Statistical comparisons between three or more groups were performed with ordinary one-way ANOVA with Tukey’s multiple comparisons test, *p<0.05, **p<0.01, ***p<0.001, ****p<0.0001. ANOVA, analysis of variance; IT, immunotoxin; PBMCs, peripheral blood mononuclear cells; PHA, phytohaemagglutinin; SSc, systemic sclerosis.

As we achieved specific elimination of the potentially pathogenic CD7⁺ T cells and NK cells, we next evaluated whether this depletion exhibits therapeutic relevance. Fibrosis accompanied by skin tightening is the main disease hallmark of SSc, so we developed a novel 3D collagen fibroblast: immune cell coculture hydrogel model that enables to study fibroblast contractility (figure 4E). In this model, spontaneous fibroblast contraction happened in the presence of allogeneic PBMCs and the level of contraction was significantly larger in the presence of PHA-activated PBMCs. PHA upregulates CD3 and CD7 expression on T cells and CD7 on NK cells (online supplemental figure 6F,G), so this model mimics the effector functions of the potentially pathogenic immune cell subsets on fibroblasts in vitro. Fibroblasts that were cocultured with sorted CD7⁺ T cells and NK cells exhibited increased contractility and a higher expression of IL-6, collagen type 1 and alpha-smooth muscle actin compared with fibroblasts cocultured with CD7⁻ cells (online supplemental figure 7). Next, we pretreated PHA-activated PBMCs with 0.33 nM a-CD3/CD7 antibodies or CD3/CD7-IT and showed that only on immunotoxin treatment, fibroblast contraction was significantly reduced compared with PHA-activated PBMCs (figure 4E). Under these conditions (24 hours of coculture), the percentage of necrotic CD8⁺ or CD56⁺ cells was not (yet) significantly affected (online supplemental figure 6H). However, we observed a sharp increase in apoptotic CD8⁺ and CD56⁺ cells (figure 4F). Interestingly, fibroblasts that were cocultured with CD3/CD7-IT treated PBMCs exhibited a decreased gene expression of COL1A1, FN1 and ACTA2 (figure 4G), indicating a lowered profibrotic phenotype.

Administration of bispecific CD3/CD7-IT treatment in the first patient with SSc effectively eliminates pathogenic CD7+ cells in blood and skin

A 34-year-old male patient with severe diffuse cutaneous SSc showed disease progression following autologous hematopoietic stem cell transplantation (ASCT) that did not respond to treatment with mycophenolate mofetil, prednisone and rituximab. The patient had developed severely invalidating diffuse skin fibrosis (a modified Rodnan skin score of 27), joint contractures, high inflammation parameters with ESR 49 mm/hour (<15 mm/hour) and C reactive protein (CRP) 78 mg/L and joint contractures. He was bedridden with a very poor prognosis and was, therefore, treated with CD3/CD7-IT as last resort. Treatment resulted in a depletion of circulating and skin-resident T cells and NK cells, and a normalisation of CRP levels from 131 mg/L to 27 mg/L after 4 weeks, which CRP levels then further decreased to normal after 5 months. His functional status stabilised, with an observed increase in quality of life, yet with a persistent invalidation due to severe skin tightening and joint contractures that proved irreversible. The patient died 1.5 years after CD3/CD7-IT treatment from disease complications.

Biological responses to CD3/CD7-IT treatment were measured with flow cytometry in patient’s blood and multiplex immunofluorescent staining in skin predrug and postdrug administration. Consistent with the expected in vitro effect, treatment with CD3/CD7-IT directed a profound elimination of circulating T cells and NK cells. Already 1 week after administration, the amount of circulating T cells and NK cells was reduced by 86% and 77%, respectively (figure 5A). CD8⁺ T cells were preferentially targeted by CD3/CD7-IT compared with CD4⁺ T cells. More specifically, the percentage of CD8⁺ T cells exhibited a 37-fold decrease while CD4⁺ T cells showed an 8-fold reduction (figure 5B). We further explored the killing efficacy of CD3/CD7-IT towards effector cytotoxic T cell and NK cell populations. Effector cytotoxic T cells were characterised as CD8⁺Perforin⁺ and effector NK cells as CD56⁺Perforin⁺. Interestingly, both CD8⁺Perforin⁺ and CD56⁺Perforin⁺ cell populations were completely depleted (100%) in patient’s blood (figure 5C). The therapeutic effectiveness towards skin-resident T and NK cells was then evaluated with multiplex immunofluorescence staining of skin biopsies before and after treatment. Post-treatment, skin biopsies showed a remarkable reduction in immune cell infiltration (figure 5D). More specifically, absolute cell counts of CD3⁺ T cells, CD8⁺ T cells and CD56⁺ NK cells were all considerably reduced post-treatment. Importantly, the numbers of CD3⁺FOXP3⁺ regulatory T cells and CD20⁺ B cells were not affected (figure 5E). While the treatment outcome was considered positive and clinically meaningful, we expect even greater benefit when CD3/CD7-IT is applied earlier in the course of the disease, when the inflammatory component is more prominent and the fibrotic process not yet irreversible.

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Figure 5

Treatment with anti-CD3/CD7-immunotoxin (CD3/CD7-IT) depletes cytotoxic T cells and NK cells in an early dSSc patient’s blood and skin. Percentage of (A) CD3⁺ T cells and CD56⁺ NK cells (B) CD4⁺ T cells and CD8⁺ T cells (C) CD8⁺Perforin⁺ T cells and CD56⁺Perforin⁺ NK cells in SSc patient’s peripheral blood before and after treatment with a-CD3/CD7-IT. Values are represented as percentage of total live peripheral blood mononuclear cells (PBMCs). (B) (right) Ratio of CD4⁺/CD8⁺ T cells before and after treatment with a-CD3/CD7-IT. (D) Representative immunofluorescent images and (E) quantification of lymphocyte subsets in the patient’s affected skin before versus after treatment with a-CD3/CD7-IT.