Background
Although short-term renal allograft survival has improved over the past decades, long-term graft survival is still limited with overall 5- and 10-year graft survival rates of 77 and 56% respectively in Europe [
1]. Research efforts have therefore focused on identifying ways to prolong graft survival. A multitude of factors are responsible for chronic allograft failure, including concomitant disease, calcineurin-inhibitor (CNI) toxicity, recurrent or de novo renal disease, as well as chronic allograft rejection [
2]. Among these factors, chronic rejection most frequently causes graft failure [
2,
3]. In this context, subclinical inflammation in renal allografts [
4‐
6] and the serological appearance of de novo donor-specific antibodies (
dnDSA) have been strongly implicated as factors for reduced graft survival [
3,
7‐
9]. A major cause for the formation of de novo DSA is non-adherence to immunosuppressive therapy [
3], and numerous studies show that non-adherence itself is a risk factor for reduced graft survival [
10‐
12].
Antibody mediated rejection (ABMR) is known to be a major contributor to graft loss [
3]. Histologically, the hallmark feature of chronic antibody mediated rejection is transplant glomerulopathy (TG), which has been shown to correlate with the formation of DSA and specific patterns of C4d deposition [
13]. Interstitial fibrosis and tubular atrophy (IF/TA), though non-specific, frequently accompany TG in chronic ABMR. Another histopathological feature, which has been observed in chronically rejected grafts, are B cell rich tertiary lymphoid organs (TLO) [
14], which have also been found in other types of chronically inflamed tissues.
Since
dnDSA and ABMR are prominent causes of graft failure, increasing attention has been drawn to B cells, due to their function as antibody-producers, as well as regulatory functions, such as cytokine production. However, so far B cells have not been specifically targeted by standard immunosuppressive protocols in renal transplantation, apart from some special applications, such as ABO-incompatible renal transplantation. Furthermore, the benefit of B cell depleting agents, such as Rituximab, in the treatment of ABMR remains controversial [
15]. Other B cell targeted therapies have been developed for chronic inflammatory and autoimmune diseases [
16,
17], but their contribution in allogeneic solid organ transplantation is still under scrutiny.
Previously, we reported on a notable difference in the relative infiltration of B-lymphocytes in the context of allogeneic vs. syngeneic transplantation in a rat kidney transplant model [
18]. In the current study, we used a rat model reflecting non-adherence to immunosuppressive therapy, to answer to following questions: 1.) to what extent can non-adherence cause rejection 2.) what effect does non-adherence have on infiltrating leukocyte populations 3.) how are chemokine transcription patterns affected 4.) how are intra-renal B-cells affected and 5.) does non-adherence result in the development of donor specific antibodies?
To this end, we used a MHC-mismatched rat model of allogeneic renal transplantation.
Methods
Animals/experimental renal transplantation
Animal experiments were performed according to German animal protection laws and NIH’s laboratory animal care principles. Study approval was granted by the inspecting authority (Regierung der Oberpfalz). A MHC-mismatched rat kidney transplantation model was used, as previously described [
19]. Male Brown Norway rats (BN) served as donors and male Lewis rats (LEW) as recipients (Charles River Laboratories, Sulzfeld, Germany, 200–250 g). Kidney transplantation was either syngeneic (Lewis-to-Lewis) or allogeneic (Brown-Norway-to-Lewis).
Kidney transplantation (Tx) was performed as previously described [
19]. In brief, left BN kidneys were explanted, flushed with cold saline and transplanted orthotopically in Lewis rats by end-to-end anastomosis of the ureter and blood vessels. Cold and warm ischemia times were approximately 35 and 30 min, respectively. Nephrectomy of the right kidney was performed at the end of the surgery.
All animals with allogeneic transplantation were treated with cyclosporine A (CyA 5 mg/kg body weight; Neoral, Novartis, Basel, Switzerland), administered once daily by gavage. In one group, CyA was administered only on alternating days after day 6, in analogy to non-adherence to immunosuppressive therapy (“Tx d28 CyA alt.”). Rats were sacrificed 6 and 28 days after transplantation. In general, syngeneic transplantation was used as a control, except for complement-dependent-cytotoxicity assay, where Lewis rat serum from day 0 was used.
Groups were abbreviated as follows:
Syngeneic transplantation sacrificed on day 6 (SynTxd6), allogeneic transplantation with daily CyA sacrificed on day 6 or day 28 (Txd6CyA, Txd28CyA), and allogeneic transplantation with CyA administered on alternating days, sacrificed on day 28 (Txd28CyAalt). Groups consisted of 6 to 11 animals.
Harvested organs were divided into quarters and either fixed in paraffin or snap-frozen in N2 and stored at −80 °C, or processed for flow cytometry.
Histology, Immunohistochemistry and Immunofluorescence
Paraffin sections were prepared from rat kidneys as previously described [
20]. After staining with hematoxylin and eosin (HE) and periodic acid schiff (PAS) stains, the histomorphological alterations were classified according to the Banff classification [
21] by an experienced pathologist.
Immunohistochemistry was performed on 3 μm formalin-fixed, paraffin-embedded sections as previously described [
18]. Primary antibodies included polyclonal rabbit anti-rat CD3 antibody (1:100, Abcam, ab5690, Cambridge, UK), polyclonal goat anti-rat CD20 antibody (1:100, Santa Cruz, sc-7735, Heidelberg, Germany), monoclonal mouse anti-rat CD68 antibody (1:150, Serotec, MCA341GA, Oxford, UK), rabbit anti-rat C4d antibody (Hycultec, HP8034, Beutelsbach, Germany), goat polyclonal anti-CCL21 / SLC antibody (aa24–133) (LS-C150160, Lifespan Biosciences, Seattle, USA), rabbit monoclonal anti-CCR7 antibody (Y59, ab32527, Abcam, Cambridge, UK). Secondary antibodies were goat anti-rabbit-biotin (Dianova, 111–065-144, Hamburg, Germany), mouse anti-goat-biotin (Dianova, 205–065-108, Hamburg, Germany), donkey anti-mouse-biotin (Dianova, 715–065-150, Hamburg, Germany). Staining was done using DAB (0.4 mg/ml, Sigma, D5637, St. Louis, USA) and AP-RED (Zytomed, ZUC001–125, Berlin, Germany). For CCL21 staining, anti-goat-Polymer-HRP Kit (Vector laboratories, Immpress Reagent Anti-Goat Ig HRP, MP-7405, Peterborough, UK) was used as a secondary antibody. C4d staining was enhanced using AP-One-Step Polymer (Zytomed, ZUC068–006, Berlin, Germany) with Permanent AP RED Kit (Zytomed, ZUC001–125, Berlin, Germany) as secondary antibody. For CCL21 and CCR7, two to three sections from randomly selected rats from each group were stained.
CD20, CD3, and CD68 staining was analyzed using Histoquest
® software. Digital pictures were taken and 10 high power fields (HPF) per specimen were examined for analysis (original × 400, covering an area of 296 μm × 222 μm) of each graft as previously described [
18]. Using Histoquest® software, the number of CD68
+, CD20
+, and CD3
+ cells were counted in relation to all cells within a defined area. Furthermore, we used immunofluorescence to better visualize the distribution of CD20
+ cell population within the grafts on formalin-fixed, paraffin-embedded materials.
Immunofluorescence staining for CD20 was performed as previously described [
20] on 1–2 randomly selected sections from each experimental group. Sections (4 μm) were deparaffinized and rehydrated. Antigen retrieval was performed in a decloaking chamber (Biocare Medical, Pacheco, USA) by treatment in citrate buffer and Antigen Unmasking Solution (Linaris, H-3300, Dossenheim, Germany). Sections were blocked using Superblock Solution (Pierce Technology, 37,515, Rockford, USA). The polyclonal goat anti-rat CD20 antibody (1:100, Santa Cruz, sc-7735, Heidelberg, Germany) was used at 1:100 in PBS overnight. After subsequent washing steps, the tissue was incubated with the donkey anti-goat-FITC antibody (1:500 in PBS, Dianova, 705–095-147, Hamburg, Germany) for 1 h at room temperature. Cell nuclei were stained using Hoechst 33,342 (Molecular Probes H-1399, Waltham, USA) 1:50,000 in PBS for 2 min. at room temperature. Sections were assessed and images taken using a Zeiss observer Z.1 Fluorescence microscope at 20× magnification. Staining specificity of anti-CD20, anti-CD3, and anti-CD68 antibodies was confirmed by anatomical staining pattern of B, and T cells, and monocytes/macrophages respectively in immunofluorescence of rat spleen sections, showing CD20-positive B cell zones and CD3-positive T cell zones in splenic follicles, as well as dispersed distribution of CD68-positive macrophages in the splenic red pulp (Additional file
1 and Additional file
2). A facs co-stain of rat monocyte/macrophage marker CD11b/c (mouse anti-rat CD11b/c-PE, eBiosciences 12–0110-82, San Diego, USA) and CD68 is also presented in the additional files section (Additional file
3). T cells were stained using rabbit anti-rat/hu/ms CD3 (5690, Abcam, Cambridge, UK) and donkey anti-rabbit-Cy5 (Dianova, 711–175-152) as secondary antibody (Additional file1) or donkey anti-rabbit-biotin (Dianova, 711–065-152) and Strep-594 (Dianova, 016–580-084) (Additional file
2). B-cells were stained using mouse anti-rat CD20 (SantaCruz, sc-393,894) and goat anti-mouse(IgM)-biotin (ThermoFisher, 31,804) as a secondary antibody with strep-Cy3 (Dianova, 016–160-084) (Additional file
1) or using goat anti-rat CD20 (SantaCruz, sc-7735) and donkey anti-goat-FITC (Dianova, 705–095-147) (Additional file
2). Macrophages were stained using mouse anti-rat CD68 (BioRad, MCA341GA) and donkey anti-mouse-DyLight 650 (Abcam, ab98797) as a secondary antibody.
Flow Cytometry
Rat spleen was mechanically macerated to yield single cell suspensions for antibody staining and flow cytometry. Spleen was coarsely chopped using a scalpel, then passed through a 70 μm cell strainer, washed, and then passed through a 30 μm filter. The cell suspension was further separated using ficoll gradient centrifugation. The white cell layer (buffy coat) was collected and used for FACS staining. Cells were blocked using 10% BSA PBS. The following antibodies were used: mouse anti-rat CD11b/c-PE (eBiosciences 12–0110-82, San Diego, USA) and mouse anti-rat CD68 (BioRad, MCA341GA) with secondary antibody donkey anti-mouse-DyLight 650 (Abcam, ab98797).
Masson Trichrome staining
Renal tissues were fixed in 4% paraformaldehyde and embedded in paraffin, cut into 4-μm thick sections and stained with hematoxylin and eosin (HE) and Masson’s trichrome (MT) staining as follows. First, sections were deparaffinized and rehydrated by treatment with decreasing percentages of ethanol and rinsing in deionized water. Sections were then treated with Bouin’s solution containing Pikrin acid, 5% acetic acid and 10% formaldehyde overnight and then rinsed. This was followed by 5 min. of Weigerts iron-hematoxylin solution in order to stain cell nuclei dark blue. Then Bieberich-Scarlet red acid-fuchsin was applied for 5 min. to stain cytoplasms red. Phosphorus tungsten and phosphorus molybdenic acid was applied for 5 min., followed by Anilin blue solution for 15 min., 1 min of 1% acetic acid, and after rinsing with water, sections were dehydrated using ethanol treatments in increasing concentrations. The morphological changes were examined under a Zeiss Axiostar microscope equipped with a digital camera and analyzed by Metamorphe software (Metamorph 4.6 Universal Imaging Corporation). Depending on the size of the tissue section 10 to 20 images per section (×20 magnification) were captured along the renal cortex, in order to calculate the total percentages of the fibrotic areas for each section.
Real-time PCR
After homogenization of frozen tissue sections using RNeasy MiniKit® (cat. 74,106, Qiagen, Hilden, Germany) total RNA was extracted, with additional DNase digestion to remove all traces of genomic DNA. Total RNA was reverse transcribed into cDNA: cDNA probes were synthesized in 20 μL reaction volume with 1 μg total RNA, 0.5 μg oligo(dT) primer (Promega, Mannheim, Gemany), 40 units of RNasin (Promega, Mannheim, Germany), 0.5 mM dNTP (Biolabs, Frankfurt am Main, Germany), 4 μL 5× transcription buffer and 200 units of Moloney murine leukemia virus (M-MLV) reverse transcriptase (Promega, Mannheim, Germany) for 1 h at 37 °C. In parallel, no-RT and no-template controls were performed. RT-PCR was performed on ViiA7 detection system in triplicates (Applied Biosystems, Darmstadt, Germany) using QuantiTect SYBR Green PCR Kit (Qiagen, Hilden, Germany). Hypoxanthine-guanine-phosphoribosyl-transferase (HPRT) was used as reference gene. All water controls were negative for target and housekeeper. The sequences of the primers were: rHPRT forw: 5’-CTTTGGTCAAGCAGTACAGCC-3′; rHPRT rev: 5’-TCCGCTGATGACACAAACATGA-3′; rCCL2 forw: 5’-ATGCAGTTAATGCCCCACTC-3′; rCCL2 rev: 5’-TTCCTTATTGGGGTCAGCAC-3′; rCCL5 forw: 5’-CTGCCCCTACTTGTCATGGT-3′; rCCL5 rev: 5’-AGATGAGCCTCACAGCCCTA-3′; rCCR5 forw: 5’-CTATGCCCTTGTTGGGGAGA-3′; rCCR5 rev: 5’-TCCTGTGGACCGGGTATAGA-3′, rCXCL13 forw: 5’-GCAAAAATCAGGCTTCCAGA -3′; rCXCL13 rev: 5’-GGGTCACAGTGCAAAGGAAT-3′; rCCL19 forw: 5’-AGACTGCTGCCTGTCTGTGA-3′; rCCL19 rev: 5’-GCTGGTAGCCCCTTAGTGTG-3′; rCCL20 forw: 5’-CAACTTTGACTGCTGCCTCA-3, rCCL20 rev: 5’-CGGATCTTTTCGACTTCAGG-3; rCCR7 forw: 5’-GGTCATTTTCCAGGTGTGCT-3, rCCR7 rev: 5’-AGTTCCGCACATCCTTCTTG-3; rLymphotoxin-β forw: 5’-TATCAC TGTCCTGGCTGTGC-3′, rLymphotoxin-β rev: 5’-GAGATGCACGAGGGTTTGTT-3′; rCCL21 forw: 5’-ACTGCAGGAAGAATCGAGGA-3′; rCCL21 rev: 5’-TGGACTGTGAACCACTCAGG-3′; rBAFF-R forw: 5’-GTGGGTCTGGTCAGTCTGGT -3′; rBAFF-R rev: 5’-CATTTTCCAGGGACTCTTGG-3′; rBAFF forw: 5’-CTGGAAACTGCCATGCTTCT-3′; rBAFF rev: 5’-TTCGTATAGTCGGCGTGTTG-3′; rIgG forw: 5’-CATTCCCTGCCCCCATC-3′; rIgG rev: 5’-CCGTTCATCTTCCACTCCGT-3′. rCXCL12 forw: 5’-CTGCCGATTCTTTGAGAGCC-3′; rCXCL12 rev: 5’-TTCGGGTCAATGCACACTTG-3′; rCXCR4 forw: 5′- TCTGAGGCGTTTGGTGCT-3′; rCXCR4 rev: 5’-CAGACCCTACTTCTTCGGA-3′. cDNA quantity was determined using a standard curve. Quantity values of target genes were normalized to the house-keeping gene HPRT, and x-fold change of normalized target gene values compared to syngeneic Tx d6 (used as calibrator) was calculated.
Quantification of donor-specific antibodies (DSA)
Donor (Brown Norway) splenocytes were isolated by macerating spleen through a 100 μm and 40 μm cell strainer, followed by ficoll centrifugation and collection of the white cell layer. Recipient serum was heat-inactivated (56 °C for 30 min.) in order to disable complement factors. Donor splenocytes were incubated with recipient serum for 30 min at 4 °C and then washed. Cells were then stained using either monoclonal mouse anti-rat IgM-PE (eBioscience, 12–0990, San Diego, USA) or polyclonal chicken anti-rat IgG-AlexFluor647 antibody (Invitrogen/Thermo Fischer, A21472, Waltham, USA). As positive controls, we incubated donor splenocytes with heat-inactivated goat or rabbit serum and stained for either goat (donkey anti-goat IgG-DyLight 650, Abcam 96,938, Cambridge, UK) or rabbit (donkey anti-rabbit IgG-Cy5, Dianova, 711–175-152, Hamburg, Germany) antibody. Finally, cells were stained for CD3-FITC (eBioscience 11–0030, San Diego, USA) and measured by flow cytometry. Data is shown for CD3+-gated cells, in order to avoid skewing of data by Fc-receptor binding of non-specific antibodies.
Complement-dependent Cytotoxicity assay (CDC)
Donor splenocytes were isolated as above and resuspended in RPMI1640 Medium (Gibco/Thermo Fischer, Waltham, USA) containing 10% inactivated FCS and 1%Penicillin/Streptomycin. Heat-inactivated recipient serum and donor splenocytes (200,000 cells/well) were incubated at 4 °C for 30 min. Rabbit complement (BAG 7018, Lich, Germany) was added and incubated for 2 h at 24 °C. Goat (DAKO X0907, Hamburg, Germany) or rabbit (DAKO X0902, Hamburg, Germany) serum were used as positive control. Cells were washed and stained with propidium iodide (PI) (Invitrogen/Thermo Fischer, Waltham, USA) to distinguish dead cells and then measured by flow cytometry. Complete lysis was measured using FixPerm (Thermo Fischer, Waltham, USA). Percent cytotoxicity was calculated using the formula: (“PI+cells in sample” – “PI+cells in medium”)/(“PI+cells in FixPerm” – “PI+cells in Medium”) ×100.
Statistical analysis
Values are provided as mean ± SEM. Statistical analysis was performed by the non-parametric Mann-Whitney U-test. p < 0.05 was considered to be statistically significant.
Discussion
Since non-adherence to immunosuppressive therapy is strongly associated with donor-specific antibodies and accelerated graft failure, our aim was to utilize a rat model of non-adherence in order to study the immunological mechanisms underlying chronic allograft injury.
In our model, MHC-mismatched rat strains were used for allogeneic renal transplantation. Acute humoral and cellular rejection was observed at day 6. As the animals were not pre-sensitized, the immunological risk was considered low, and no induction therapy was used. When immunosuppression was continued, rejection subsided in some animals, but not all, probably because the dose of cyclosporine used (5 mg/kg) was relatively low and no induction therapy or steroid was administered on top. Under daily cyclosporine administration, normal histology or mild cellular rejection was seen at day 28. In contrast, the non-adherence group suffered from a significant increase in the rate of cellular rejection with additional features of acute humoral rejection – illustrated by initiation of peritubular capillaritis. Our model intended to show mechanisms of early chronic parenchymal changes. Such changes were indeed induced in our model of non-adherence, as demonstrated by a significant increase in interstitial fibrosis.
While cellular infiltration was minimal after syngeneic transplantation, high numbers of inflammatory cells were seen early after allogeneic transplantation (day 6) with monocytes dominating the infiltrate. The numbers of monocytes, T cells and B cells declined when standard immunosuppression with daily CyA was continued. However, under conditions simulating non-adherence, T cell infiltration did not resolve as quickly as under daily immunosuppression. Meanwhile, B cell numbers remained elevated in comparison to syngeneic transplantation and monocyte numbers declined to a level similar to that after syngeneic transplantation. In line with these results, Hueso et al. previously showed that early interstitial fibrosis/tubular atrophy (IF/TA) and reduced graft survival are associated with increased infiltration of T and B cells in human renal transplant biopsies [
25].
The changes seen in the pattern of intra-renal chemokine transcription mirrored the changes in the composition of the cellular infiltrate, with chemokines attracting T and B lymphocytes, such as CCL19, CCL20, CCL21, CCL5 and lymphotoxin-β, increased in non-adherence.
Interestingly, CCL19, CCL20, and CCL21, were much more strongly induced in the setting of non-adherence than during the initial inflammatory reaction early after Tx (d6). CCL19, CCL21, and their receptor CCR7 are known to regulate homing and co-localization of dendritic cells and naïve T cells in lymphoid organs and are essential to T cell sensitization and the formation of an adaptive immune response [
26]. However, they have also been implicated in the formation of tertiary lymphoid organs (TLO) in the context of chronic inflammation [
24,
27,
28]. These structures have also been found in transplant organs and are associated with a poorer outcome [
14,
29]. In a murine model of kidney transplantation, the fusion protein CCL19-IgG, which interferes with normal CCL19-CCR7 signaling, was found to strongly reduce graft rejection [
30]. In our model of non-adherence, chemokines associated with TLO formation are strongly expressed, and this is accompanied with the formation of dense lymphocyte aggregates.
Another factor that has been associated with chronic inflammation and formation of B cell rich TLO is B cell activating factor (BAFF) [
31]. BAFF is an activation, maturation and survival factor for B cells, expressed by lymph node stromal cells, neutrophils, macrophages, monocytes, dendritic cells and T cells [
32]. A pathogenetic role for BAFF has been suggested for several autoimmune diseases, including Sjögren Syndrome, systemic lupus erythematosus, and multiple sclerosis [
33‐
35]. In the context of renal transplantation, higher serum levels of BAFF are associated with donor-specific antibodies [
36], blood cell-bound BAFF with worse renal graft function, and intra-graft BAFF expression is associated with ABMR and IF/TA [
37]. We now show that BAFF transcription is increased within the graft during non-adherence. In line with this, IgG transcription levels are also increased during non-adherence. In fact, the non-adherence group was the only group that showed intra-renal IgG transcription, demonstrating that local intra-graft antibody formation exclusively occurred after prolonged suboptimal immunosuppression.
Although, fully developed TLO structures were not yet observed in our experimental setting at the analyzed time-points, the enhanced organization of B lymphocytes into dense clusters during our simulation of non-adherence together with the increased expression of TLO-associated chemokines CCL19, CCL20, CCL21, and BAFF may be indicative of early steps in the formation of these highly organized structures. Furthermore, the appearance of intra-graft IgG transcription maybe linked to the development of an organized local adaptive immune response. Although our experiments cannot differentiate plasma cell infiltration from local differentiation from precursor cells, a possible explanation maybe that BAFF activates intra-renal B cells, which mature into antibody-secreting plasma cells within the graft. Similarly, our experiments cannot rule out that increased IgG transcription is due to turnover of local B cell populations in non-adherence, but evidence for local antibody production by plasma cells in chronic rejection has been provided by Thaunat et al. [
14]. There is also evidence for clonal expansion of B cells inside grafts [
38]. No conclusions can be drawn as to the specificity or diversity of the IgG produced in our non-adherence model, and further experiments will be needed to establish the source and specificity of intra-graft IgG production. Others have shown however, that locally and systemically produced antibodies differ in diversity and timing with more diverse HLA (human leukocyte antigen) specificities being generated from intra-graft antibody production [
14,
39].
In our model, de novo DSA were detected in rat serum under conditions mimicking non-adherence to therapy. This corresponds to data from studies of renal transplant patients [
3,
10,
11]. Antibodies were shown to be donor-specific, since binding of recipient Lewis rat splenocytes did not occur. Although our experiments could not specifically identify anti-MHC antibodies, endothelial non-MHC targets for these antibodies were unlikely since splenocytes were used in our assay. IgM and IgG DSA were detected early after transplantation (day 6), following a kinetic previously described for rat humoral responses after immunization [
40,
41]. At the later timepoint, we saw a clear induction of a secondary humoral response, where IgM was no longer detected, while IgG levels remained elevated. We interpreted this as a sign that Ig class switching was completed, and that sensitization to donor antigens and initial DSA production takes place very early. Our results suggest that activated B cells and plasma cells are then armed and ready for antibody production, and are kept in check by appropriate immunosuppression with CNI. Analysis of CDC showed that DSA were cytotoxic early after Tx (d6), but not after non-adherence or daily CyA (d28), which was consistent with the pattern of C4d-staining observed in the different groups. Our experiments do not offer a specific mechanism to explain this phenomenon, but one possibility is that the different immunosuppressive treatments and durations result in a switch in the IgG-subclass generated and thereby also determine the phenotype of ABMR, eg. C4d-positive vs. C4d-negative, in line with recently published observations of DSA IgG subclasses and rejection phenotypes in transplant patients [
42]. In this study of renal transplant patients, chronic ABMR was associated with the non-complement activating IgG subclass IgG4 in humans, whereas acute ABMR was associated with the complement-fixing IgG3 [
42].
Under-immunosuppression in a clinical setting may be due to non-adherence to therapy or to inter-individual variations in responsiveness to CNI, since CNI therapy is monitored using serum concentration, not functional tests. Considering this, even when optimal adherence to therapy is achieved, a group of patients may still effectively be “under-immunosuppressed” and at risk of chronic rejection.
While there is a lot of data showing the deleterious effects of DSA on graft outcome, there is an ongoing debate over which DSA are clinically relevant, or more precisely, what features of DSA, such as MFI (mean fluorescence intensity), complement-fixing capacity or IgG-subclass, are linked to deleterious outcomes and require treatment [
42‐
44]. Our model offers an ideal framework for deciphering such critical issues.
Several animal models have been established in which preformed DSA are induced using pre-transplant immunization [
45,
46]. Since in the majority of cases, DSA are de novo DSA and not DSA from pre-sensitization, our model - with reliable histological and serological entities of acute antibody mediated rejection during non-adherence - more closely resembles this highly prevalent group of patients.