Cytotherapy

BackgroundVascularized composite allotransplantation has become a viable reconstructive option for selected patients, but preservation remains a major barrier to broader clinical application. Static cold storage is the current gold standard, yet ischemia reperfusion injury and limited preservation times restrict its effectiveness. Recent advances in machine perfusion and subzero non-freezing storage (or supercooling) have prompted renewed interest in optimizing graft viability. MethodsFollowing PRISMA guidelines, we systematically searched PubMed, EMBASE, and Cochrane, covering studies published from June 2022 through August 2025 for studies on ex vivo preservation of vascularized composite allotransplantations. Eligible articles included original studies in English evaluating postharvest, pretransplant preservation strategies. Data extracted were study design, preservation methods, perfusates, and primary outcomes. Risk of bias was assessed using SYRCLE for animal studies and JBI for human/cadaver studies. ResultsSeventeen studies met inclusion criteria: one on static cold storage, thirteen on machine perfusion, and three on supercooling. Static cold storage research has declined, with the only recent study investigating sub-normothermic machine perfusion as a recovery adjunct. Machine perfusion studies focused on optimization of perfusion parameters, perfusate composition, and circuit design. Red blood cell-based perfusates remained common, but alternative oxygen carriers such as polymerized hemoglobin-based oxygen carrier-201 and dextran oxygen microcarriers showed promise despite edema-related challenges. Supercooling studies demonstrated feasibility of multi-day preservation in rodent and porcine models. Overall, risk of bias was high or unclear across animal studies, mainly due to selection and performance bias, whereas the single human ex vivo study showed low risk of bias. ConclusionsThe field of vascularized composite allograft preservation is expanding rapidly, with machine perfusion and supercooling emerging as the most promising strategies to extend graft viability beyond the limits of static cold storage. However, translation to clinical setting remains limited by small preclinical studies, methodological heterogeneity, and the paucity of functional and immunologic endpoints. Standardized protocols, robust large-animal models, and eventual human feasibility trials are needed to establish clinically applicable preservation strategies. Level of evidence: IV

BackgroundThe homozygous ADA2: c.506G>A (p.Arg169Gln; p.R169Q) variant accounts for majority of Deficiency in Adenosine Deaminase 2 (DADA2). This monogenic disorder may be amenable to ex vivo gene therapy by correcting the pathogenic mutation in CD34+ hematopoietic stem and progenitor cells (HSPCs). ObjectiveTo apply CRISPR-Cas9 and homology-directed repair (HDR) as a surrogate strategy to model correction of the pathogenic ADA2 c.506G>A variant in healthy cord blood HSPCs. MethodsHSPCs were electroporated with optimised CRISPR-Cas9 editing reagents, and editing outcomes, including HDR and on-target deletions, were quantified by ddPCR. Cell functionality was assessed through colony-forming unit (CFU) assays and by xenotransplantation into NOD SCID Gamma (NSG) mice. Two HDR enhancement strategies were tested: (1) genetic inhibitors of p53 and non-homologous end joining (NHEJ) pathways, and (2) pharmacological NHEJ inhibition. ResultsSmall-molecule NHEJ inhibitors increased HDR efficiency approximately two-fold (from [~]40 % to [~]80 %). Edited HSPCs retained normal CFU capacity and successfully engrafted in NSG mice. However, up to 8 % of edited cells exhibited on-target chromosome loss, though this declined over time. Up to 40 % of T cells and fibroblasts demonstrated similar losses under NHEJ inhibitors treatment. In contrast, genetically encoded inhibitors did not improve HDR. ConclusionThe ADA2 p. c.506G>A variant can be effectively edited employing surrogate strategy in HSPCs without impairing functionality. Although pharmacological inhibition of NHEJ enhances HDR efficiency, it also increases the risk of on-target chromosome aberrations, highlighting the need for careful consideration of the associated risks and benefits in therapeutic gene editing. Key messages1) The ADA2 p.R169Q variant can be efficiently corrected via HDR, and the edited CD34+ HSPCs retain their engraftment capability in NSG mice. 2) Pharmacological inhibition of NHEJ using small-molecule inhibitors increases HDR efficiency but is associated with significant on-target deletions and chromosomal arm loss, particularly in differentiated cell types, and in a donor-dependent manner. Capsule summaryThe ADA2 p.R169Q variant is a viable target for precision gene editing in hematopoietic stem cells. Although inhibition of NHEJ improves HDR efficiency, it concomitantly increases the risk of large on-target deletions, particularly in differentiated cells.

Background and AimGamma delta T cells are multivalent immune cells with innate and adaptive features that sense a broad spectrum of tumor-associated stress patterns to lyse them without prior potentiation. They are therefore a good option for developing an off-the-shelf therapeutic immune cell product with antitumor functions. Therefore, we aimed to develop an optimized cGMP compatible protocol for expanding V gamma 9-V delta 2 T cells in a serum-free media for adoptive immunotherapy applications. Methods and ResultsPeripheral blood mononuclear cells (PBMC) from healthy donors were activated with Zoledronic Acid (ZOL) and IL-2 for 14 days. Cell proliferation, fold expansion, and phenotype were monitored. Among the regular donors, the baseline levels (day 0) of CD3+Vgamma9+delta2+ T cells were (05.10+/-0.74%). There was a robust expansion of V gamma 9-V delta 2 T cells in the serum-free media (110+/-29.89-fold). During processing, an abrupt reduction of {beta} T cells was observed as early as day +07. After two weeks, 87.82+/-5.11% (n=8) of T cells were CD3+Vgamma9+ in Optimizer with 97.15+/-0.7% of the CD3+Vgamma9+ T cells positive for delta2. The CD3+Vgamma9+ NKG2D+ increased during expansion, reaching 93.76+/-1.55% expression on day +14. V gamma 9-V delta 2 T cells expanded in the serum-free (Optimizer) media had relatively reduced variance and reduced over all yield and fold expansion but comparable percentage of Vgamma9+ and {beta} TCR+ T cells on day 14. A flow cytometry-based tumor-toxicity assay gauged the antitumor functions against K562 cell lines. Pretreatment of K562 cells with ZOL differentially enhanced (2.48+/-0.76 fold) the cytotoxic capacity of V gamma 9-V delta 2 T cells in a donor-dependent manner. The conditions for lentiviral transduction and transgene expressions of V gamma 9-V delta 2 T cells were improvised as gauged by GFP expression driven by CMV promoter (39.09+/- 8.94%) without compromising the viability. ConclusionWe have optimized a cGMP compatible protocol for expansion of human V gamma 9-V delta 2 T cells in a serum-free media with high purity and viability in as early as 07 days. Pretreatment of target tumor cells with ZOL enhanced the cytotoxicity, revealing the impact of V gamma 9-V delta 2 T cell intrinsic factors in tumor lysis. This protocol, may be scaled up for clinical translation for adoptive immunotherapy.

In vitro expansion of spermatogonial stem cells (SSCs) has been established using animal-derived fetal bovine serum (FBS) and bovine serum albumin (BSA). However, the use of animal components during cell culture introduces the risk of contaminating cells with pathogens, and leads to animal epitope expression, rendering them unsuitable for medical use. Therefore, this study set out to develop a xeno-free, fully defined media for the expansion of human SSCs. We show that the molecules Prostaglandin D2 (PGD-2) and Insulin-Like Growth Factor 1 (IGF-1) can replace FBS and BSA in cell culture media without loss of viability or expansion capability, and that Rho-Associated, Coiled-Coil Containing Protein Kinase (ROCK) inhibitor Y-27632 supplementation improves viability after cryopreservation. Long-term SSC cultures expanded in xeno-free, defined culture conditions shared identical protein expression profiles for well-known SSC markers, while gene expression analyses revealed a significant improvement in quiescent SSC and pan-germ markers. This xeno-free, defined formulation allows for standardized SSC culture free of animal pathogens.

BackgroundMesenchymal stromal cells (MSCs) have shown great promise in the field of regenerative medicine as many studies have shown that MSCs possess immunomodulatory function. Despite this promise, no MSC therapies have been granted licensure from the FDA. This lack of successful clinical translation is due in part to MSC heterogeneity and a lack of critical quality attributes (CQAs). While MSC Indoleamine 2,3-dioxygnease (IDO) activity has been shown to correlate with MSC function, multiple CQAs may be needed to better predict MSC function. MethodsThree MSC lines (two bone marrow, one iPSC) were expanded to three passages. At the time of harvest for each passage, cell pellets were collected for nuclear magnetic resonance (NMR) and ultra-performance liquid chromatography mass spectrometry (UPLC-MS), and media was collected for cytokine profiling. Harvested cells were also cryopreserved for assessing function using T cell proliferation and IDO activity assays. Linear regression was performed on functional and multiomics data to reduce the number of important features, and partial least squares regression (PLSR) was used to obtain putative CQAs based on variable importance in projection (VIP) scores. ResultsSignificant functional heterogeneity (in terms of T cell suppression and IDO activity) was observed between the three MSC lines, as well as donor-dependent differences based on passage. Omics characterization revealed distinct differences between cell lines using principal component analysis (PCA). Cell lines separated along principal component 1 based on tissue source (bone marrow vs. iPSC-derived) for NMR, MS, and cytokine profiles. PLSR modeling of important features predicts MSC functional capacity with NMR (R2=0.86), MS (R2=0.83), cytokines (R2=0.70), and a combination of all features (R2=0.88). DiscussionThe work described here provides a platform for identifying putative CQAs for predicting MSC functional capacity using PLSR modeling that could be used as release criteria and guide future manufacturing strategies for MSCs and other cell therapies.

Canonical HIV-1 entry into target cells depends on binding to CD4 as a primary receptor. Because of this, use of the CD4 receptor as a viral trap (a decoy receptor used to prevent infection of target cells) is a promising strategy for the treatment of HIV-1. One challenge in using CD4 viral traps is maintaining enough of the decoy receptor in circulation to remain effective. Here we present a strategy to produce cell-based CD4 viral traps by engineering hematopoietic stem and progenitor cells (HSPCs) to express the CD4 receptor in red blood cell (RBC) progeny. This takes advantage of the ability of the HSPC to repopulate the blood system for a lifetime, while leveraging the fact that RBCs greatly outnumber any cell targeted for infection. Engineered HSPCs efficiently express CD4 on their cell surface after differentiation to the RBC lineage in vitro. Fusion of CD4 to glycophorin A (GPA) and introduction of a truncated erythropoietin receptor (tEPOR) leads to increased CD4 expression and enrichment of edited cells (CD4-GPA-tEPOR) to levels capable of neutralizing HIV-1 pseudovirus in vitro. In sum, this work presents a potential strategy for the one-time delivery of CD4-RBC viral traps through autologous transplantation of engineered HSPCs.

During the last few years, gene editing has emerged as a powerful tool for the therapeutic correction of monogenic diseases. CRISPR/Cas9 applied to hematopoietic stem and progenitor cells (HSPCs) has shown great promise in proof-of-principle preclinical studies to treat haematological disorders, and clinical trials using these tools are now underway. Nonetheless, there remain important challenges that need to be addressed, such as the efficiency of targeting primitive, long-term repopulating HSPCs and expand them in vitro for clinical purposes. Here we have tested the effect exerted by different culture media compositions on the ability of HSPCs to proliferate and undergo homology directed repair-mediated knock-in of a reporter gene, while preserving their stemness features during ex-vivo culture. We tested different combinations of compounds and demonstrated that by supplementing the culture media with inhibitors of histone deacetylases, and/or by fine-tuning its cytokine composition it is possible to achieve high levels of gene targeting in long-term repopulating HSPCs both in vitro and in vivo, with a beneficial balance between preservation of stemness and cell expansion, thus allowing to obtain a significant amount of edited, primitive HSPCs compared to established, state-of-the-art culture conditions. Overall, the implantation of this optimized ex vivo HSPC culture protocol will improve the efficacy, feasibility and applicability of gene editing and will likely provide one step further to unlock the full therapeutic potential of such powerful technology.

Acute graft versus host disease (GVHD) remains a significant complication following hematopoietic stem cell transplant (HSCT), despite improved human leukocyte antigen (HLA) matching and advances in prophylactic treatment regimens. Previous studies have shown promising results for future regulatory dendritic cell (DCreg) therapies in the amelioration of GVHD. This study evaluates the effects of cryopreservation on DCreg generation, generation of young and older DCreg in serum-free media, and the feasibility of DCreg generated from young and older HSCT donor monocytes. DCreg were generated in X-vivo 15 serum-free media from donor monocytes. Donors included young and older individuals, either healthy donors or HSCT patients. Phenotypic differences in cell populations were assessed via flow cytometry while pro-inflammatory and anti-inflammatory cytokine production was evaluated in culture supernatants. The number of DCreg generated from cryopreserved monocytes of healthy donors was not significantly different from freshly isolated monocytes. DCreg generated from cryopreserved monocytes had similar levels of co-stimulatory molecule expression, inhibitory molecule expression, and cytokine production as freshly isolated monocytes. Young and older healthy donor monocytes generated similar numbers of DCreg with similar cytokine production and phenotype. Although monocytes from older HSCT patients produced significantly fewer DCreg, DCreg from young and older HSCT patients have a comparable phenotype and cytokine production. Monocytes from young and older myelodysplastic syndrome (MDS) patients generated reduced numbers of DCreg compared to non-MDS monocytes. Results suggest cryopreservation of monocytes from many HSCT patients allows for cost effective generation of DCreg for the prevention and treatment of GVHD on an as needed basis. Although generation of DCreg from MDS patients require further assessment, these data support the possibility of in vitro generated DCreg as a therapy to reduce GVHD-associated morbidity and morbidity in young and older HSCT recipients.

Successful clinical translation of mesenchymal stromal cell (MSC) products has not been achieved in the United States and may be in large part due to MSC functional heterogeneity. Efforts have been made to identify priming conditions that produce MSCs with consistent immunomodulatory function; however, challenges remain with predicting and understanding how priming impacts MSC behavior. The purpose of this study was to develop a high throughput, image-based approach to assess MSC morphology in response to combinatorial priming treatments and establish morphological profiling as an effective approach to screen the effect of manufacturing changes (i.e. priming) on MSC immunomodulation. We characterized the morphological response of multiple MSC lines/passages to an array of Interferon-gamma (IFN-{gamma}) and Tumor Necrosis Factor alpha (TNF-) priming conditions, as well as the effects of priming on MSC modulation of activated T cells and MSC secretome. Although considerable functional heterogeneity, in terms of T cell suppression, was observed between different MSC lines and at different passages, this heterogeneity was significantly reduced with combined IFN-{gamma}/TNF- priming. The magnitude of this change correlated strongly with multiple morphological features and was also reflected by MSC secretion of immunomodulatory factors e.g. PGE2, ICAM-1, and CXCL16. Overall, this study further demonstrates the ability of priming to enhance MSC function, as well as the ability of morphology to better understand MSC heterogeneity and predict changes in function due to manufacturing.

Functional testing of cytotoxic lymphocytes is essential for research and quality control (QC), but most assays require freshly prepared target cells and extensive handling. A ready-to-thaw, no-wash, flow cytometry-based cytotoxicity assay was developed using pre-labeled K562 targets cryopreserved in STEM-CELLBANKER(R) EX (SCB) as suitably sized aliquots. SCB tolerability was evaluated in K562, NK-92, and primary natural killer (NK) cells; post-cryopreservation label stability of CellTrace Violet (CTV) and carboxyfluorescein succinimidyl ester (CFSE) was assessed; freezing and thawing conditions were optimized; and wash versus no-wash workflows were compared using viability-based and absolute-count readouts, across effector-to-target (E:T) ratios with NK donors and NK-92 cells. Effector viability remained high at SCB concentrations up to 10%, and 5% SCB was selected for assay design. After cryopreservation, CTV labeling remained stable over the tested storage period, whereas CFSE showed substantial signal loss. Warm-medium thawing performed comparably to water-bath thawing, and the consolidated protocol (SCB plus fetal calf serum and thermal buffering) maintained high post-thaw target viability and recovery. In killing assays, lysis increased with increasing E:T ratios; omission of the post-thaw wash had minimal impact, and 5% SCB did not impair cytotoxic function. This ready-to-thaw workflow reduces hands-on time and sample manipulation, while improving standardization for reproducible results and enabling high-throughput functional testing and QC.

Humanized mouse models have improved biomedical research by providing a tractable system with which to perform in vivo experiments on human tissues. Use of irritators is the standard method for establishing high levels of stem cell engraftment, however not all institutes have access to this instrumentation in the animal facility. The use of busulfan has been successfully used to precondition for stem cell engraftment on a limited number of mouse backgrounds. In this report we further test the utility of busulfan as a means to successfully engraft hIL15-Tg-NSG and SGM3-NSG mouse stains which are capable of establishing the innate NK cell and myeloid immune compartments. Results from our studies show that busulfan can successfully precondition hIL15-Tg-NSG mice but not SGM3-NSG mice for high levels of human immune cell engraftment. SGM3-NSG mice preconditioned with busulfan exhibited only 10-20% human CD45 cells in the bone marrow or spleen, where as NSG and hIL15-Tg-NSG mice routinely achieved [~]80%. Busulfan preconditioned SGM3-NSG mice showed elevated levels of granulocytic MDSC, and cDC1 and cDC2 myeloid populations. This is in contrast with hIL15-TG-NSG which showed robust reconstitution of mature CD16 expressing NK cells. We conclude from our studies that busulfan is an effective means to precondition mice for CD34+ stem cell engraftment, but it may have limitations when use to precondition the SGM3-NSG model.

BackgroundAdipose-derived mesenchymal stem cells (ADSCs) have emerged as a promising therapeutic modality for cellular therapy because of their rapid proliferation and potent cellular activity compared to conventional bone marrow-derived mesenchymal stem cells (MSCs). Cosmetic lipoaspirates provide an easily obtainable source of ADSCs. Cryopreservation facilitates their clinical application due to increased transportability and pooling of sufficient numbers of cells. However, proper cryopreservation techniques have not been established yet.\n\nMethodsWe evaluated the post-thaw viability and ADSC functions after cryopreservation with three cryoprotectants (serum containing 10% dimethylsulfoxide (DMSO), serum-free: CP-1TM, DMSO-free: SCB-DFTM) at two temperature (-80{degrees}C, -150{degrees}C) and two cell densities: (1 x 106, 7 x 106 cells/mL) for up to 18 months using cryovials. After determining optimal conditions, we also tested if large quantities of ADSCs remained viable after 18 months of cryopreservation in a 100-mL cryobag. Rate-controlled freezing methods or liquid nitrogen storage were not exploited.\n\nResultsADSCs cryopreserved in serum containing 10% DMSO or CP-1TM at -150{degrees}C and 7 x 106 cells/mL were most viable (>85%) after 18 months without perturbation of MSC functions. Even suboptimal conditions (-80{degrees}C, 1 x 106 cells/mL, no DMSO) assured >80% viability when stored for up to 9 months. Large quantities of ADSCs in a cryobag were properly cryopreserved.\n\nConclusionsA programmable freezer or liquid nitrogen storage is not necessary. CP-1TM is preferable in terms of side effects. Simplified cryopreservation methods (-80{degrees}C and no DMSO) can be used for up to 9 months, resulting in reduced infusion toxicities and lower costs.

Mesenchymal stromal cells (MSCs) are currently being tested in numerous clinical trials as potential cell therapies for the treatment of various diseases and due to their potential immunomodulatory, pro-angiogenic, and regenerative properties. However, variabilities in tissue sources, donors, and manufacturing processes and the lack of defined critical quality attributes (CQAs) and clinically relevant mechanism of action (MoA) pose significant challenges to identify MSC cell therapy products with a predictable therapeutic outcome. This also hinders regulatory considerations and broad clinical translation of MSCs. MSC products are often administered to the patient immediately after thawing from cryopreserved vials (out-of-thaw). However, the qualifying quality-control assays are either performed before cryopreservation, or after culturing the post-thaw cells for 24-48 hours (culture-rescued), none of which represent the out-of-thaw product administered to patients. In this study, we performed a broad functional characterization of out-of-thaw and culture-rescue MSCs from bone marrow (BM-MSCs) and cord tissue (CT-MSCs) using macrophage activation and T cell proliferation-based in vitro potency assays and deep phenotypic characterization using single-cell RNA-sequencing. Using this data, we developed unbiased computational models, specifically symbolic regression (SR) and canonical correlation analysis (CCA) models to predict the immunomodulatory potency of MSCs. Overall, our results suggest that manufacturing conditions (OOT vs. CR) have a strong effect on MSC-function on MSC interactions with macrophages and T cells. Furthermore, single-cell RNA-seq analyses of out-of-thaw BM and CT-MSCs indicate a tissue of origin-dependent variability and heterogeneity in the transcriptome profile. Using symbolic regression modeling we identified specific single-cell transcriptomic attributes of MSCs that predict their immunomodulatory potency. In addition, CCA modeling predicted MSC donors with high or low immunomodulatory potency from their transcriptome profiles. Taken together, our results provide a broad framework for identifying predictive CQAs of MSCs that could ultimately help in better understanding of their MOAs and improved reproducibility and manufacturing control of MSCs.

Matrigel remains the gold standard substrate for culture of induced pluripotent stem cells (iPSCs). However, its highly variable composition, animal origin and unpredictable effects on biological activity have been discussed for more than 3 decades. In this study, we explore the use of fragment E8 of recombinant laminin 511, commercially available in form of iMatrix-511, as an alternative to Matrigel for iPSC maintenance and differentiation. Female iMR90-4 human iPSCs were cultured on either iMatrix or Matrigel and assessed for cell growth and viability, pluripotency, genetic stability, and ability to differentiate into isogenic brain microvascular endothelial cells (iBMECs) and brain pericytes. It was observed that iMatrix facilitated iPSC growth and viability comparable to Matrigel while maintaining a higher number of more consistently sized colonies. Additionally, like Matrigel, iMatrix maintained the expression of pluripotency markers SSEA-4 and OCT-3/4 over 15 passages without inducing DNA damage. iMatrix also supported the differentiation of these iPSCs into isogenic iBMECs and pericytes, which were successfully co-culture for generation of a simplified blood-brain barrier model. Overall, we showed that iMatrix, which is a cost effective, fully defined, and xenofree alternative can be used as a substitute for Matrigel for maintenance and differentiation of iPSCs.

Native and engineered extracellular vesicles (EVs) generated from human megakaryocytes (huMkEVs) or from the human megakaryocytic cell line CHRF (CHEVs) interact with tropism delivering their cargo to both human and murine hematopoietic stem and progenitor cells (HSPCs). 24 hours after intravenous infusion of huMkMPs into NOD-scid IL2R{gamma}null (NSG) mice, they induced a nearly 50% increase in murine platelet counts relative to saline control, thus demonstrating the potential of these EVs, which can be stored frozen, for treating thrombocytopenias. PKH26-labeled huMkMPs or CHEVs localized to the HSPC-rich bone marrow preferentially interacting with murine HSPCs. Using engineered huMkEVs or CHEVs, their receptor-mediated tropism for HSPCs was explored to functionally deliver synthetic cargo, notably plasmid DNA coding for a fluorescent reporter, to murine HSPCs both in vitro and in vivo. These data demonstrate the potential of these EVs as a non-viral, HSPC-specific cargo vehicle for gene therapy applications to treat hematological diseases. Native and engineered human megakaryocytic extracellular vesicles for targeted non-viral cargo delivery to blood stem cells (Table of Contents): O_FIG O_LINKSMALLFIG WIDTH=200 HEIGHT=111 SRC="FIGDIR/small/536479v1_ufig1.gif" ALT="Figure 1"> View larger version (49K): org.highwire.dtl.DTLVardef@664768org.highwire.dtl.DTLVardef@d9fe13org.highwire.dtl.DTLVardef@1b795eforg.highwire.dtl.DTLVardef@1d48e2d_HPS_FORMAT_FIGEXP M_FIG C_FIG Graphical Overview: Native and engineered human megakaryocytic extracellular vesicles (huMkEVs) for provide targeted non-viral cargo delivery to blood stem cells. We demonstrate that huMkEVs as a transformational cargo-delivery system to blood stem cells (hematopoietic stem and progenitor cells, HSPCs) in NOD-scid IL2R{gamma}null (NSG) mice. Intravenous delivery of native huMkEVs enhances de novo platelet biogenesis by inducing megakaryocytic differentiation of murine HSPCs, thus demonstrating the desirable strong tropism of huMkEVs for murine HSPCs. Based on this tropism, we demonstrate that engineered huMkEVs can deliver functional plasmid-DNA cargo specifically to HSPCs.

BackgroundCompetitive transplantation is essential for defining intrinsic repopulating capacity of murine hematopoietic stem and progenitor cells (HSPCs), yet comparable assays for human cells have been limited by the lack of a robust in vivo platform. MethodsHere, we describe a novel competitive transplantation method in humanized NOD.Cg-KitW-41J Tyr + Prkdcscid Il2rgtm1Wjl/ThomJ (NBSGW) mice that enables simultaneous engraftment and longitudinal tracking of distinct human grafts within a shared microenvironment. ResultsUsing human leukocyte antigen-mismatched donor CD34+ cells, this method facilitates standard flow cytometry panels to track multiple donor cell chimerism, lineage output, and HSPC composition. The experimental framework may be adapted to different mouse models, conditioning strategies, donor sources, and treatments. ConclusionsOverall, this humanized competitive repopulation assay fills a critical translational gap and offers a flexible foundation for advancing mechanistic discovery in human hematopoietic biology and improving clinical strategies for stem cell transplantation.

BackgroundBlood vessel organoids (BVOs) represent a promising tool for modeling vascular diseases, drug screening, and regenerative therapies. However, current protocols for BVO generation are complex, labor-intensive, and reliant on animal-derived extracellular matrices (ECM) such as Matrigel, limiting reproducibility, scalability, and clinical applicability. MethodsWe developed a simplified, animal-origin-free protocol for BVO generation that addresses current limitations and enables high-throughput automated workflows. The method employs ultra-low attachment 96-well U-bottom plates for standardized aggregation and differentiation of human induced pluripotent stem cells (hiPSCs) in a human derived collagen-based extracellular matrix. Unlike conventional protocols where aggregates are embedded in a two-layer ECM, our approach utilizes a single-layer, which we termed "sitting drop". This innovative approach requires considerably fewer materials and handling steps and is compatible with high-throughput automated machines. ResultsBVO generation utilizing the here described optimized protocol resulted in the formation of BVOs with reproducible morphology and cellular composition. Flow cytometry confirmed the presence of CD31 endothelial cells and PDGFR{beta} pericytes in BVOs, generated in sitting drops, with cell population percentages comparable to those observed in traditional two-layer BVO cultures. In vivo transplantation of mature BVOs in a mouse full-thickness skin wound model demonstrated successful integration of BVO derived cells into host vessels, highlighting their potential in cell-based therapies. ConclusionOur study presents a robust and animal-origin-free method for BVO generation based on single-layer "sitting drop" cultures. This protocol maintains cellular integrity while enhancing reproducibility and automation-readiness, paving the way for high-throughput screening and clinical translation of vascular organoid technology. HighlightsO_LIEntire blood vessel organoid (BVO) workflow performed in a single ultra-low attachment-96 plate C_LIO_LIFully animal-origin-free: no Matrigel or Geltrex required throughout the protocol C_LIO_LIRobust generation of BVOs using human collagen-based ECM C_LIO_LIHigh-throughput compatible and automation-ready "sitting drop" culture system C_LIO_LIIntegration of BVO-derived cells into host vessels in vivo C_LI

Widespread treatment of human diseases with gene therapies necessitates the development of gene transfer vectors that integrate genetic information effectively, safely and economically. Accordingly, significant efforts have been devoted to engineer novel tools that i) achieve high-level stable gene transfer at low toxicity to the host cell; ii) induce low levels of genotoxicity and possess a safe integration profile with a high proportion of integrations into safe genomic locations; and iii) are associated with acceptable cost per treatment and scalable/exportable vector production to serve large numbers of patients. The Sleeping Beauty (SB) transposon has been transformed into a vector system that is fulfilling these requirements.\n\nIn the CARAMBA project, we use SB transposition to genetically modify T cells with a chimeric antigen receptor (CAR) specific for the SLAMF7 antigen, that is uniformly and highly expressed on malignant plasma cells in multiple myeloma. We have demonstrated that SLAMF7 CAR-T cells confer specific and very potent anti-myeloma reactivity in pre-clinical models, and are therefore preparing a Phase I/IIa clinical trial of adoptive immunotherapy with autologous, patient-derived SLAMF7-CAR T cells in multiple myeloma (EudraCT Nr. 2019-001264-30/CARAMBA-1).\n\nHere we report on the characterization of genomic safety attributes in SLAMF7 CAR-T cells that we prepared in three clinical-grade manufacturing campaigns under good manufacturing practice (GMP), using T cells that we obtained from three healthy donor volunteers. In the SLAMF7 CAR-T cell product, we determined the average transposon copy number, the genomic insertion profile, and presence of residual SB100X transposase. The data show that the SLAMF7 CAR transposon had been inserted into the T cell genome with the close-to-random distribution pattern that is typical for SB, and with an average transposon copy number ranging between 6 and 12 per T cell. No residual SB100X transposase could be detected by Western blotting in the infusion products. With these attributes, the SLAMF7 CAR-T products satisfy criteria set forth by competent regulatory authorities in order to justify administration of SLAMF7 CAR-T cells to humans in the context of a clinical trial. These data set the stage for the CARAMBA clinical trial, that will be the first in the European Union to use virus-free SB transposition for CAR-T engineering.\n\nDisclosuresThis project is receiving funding from the European Unions Horizon 2020 research and innovation programme under grant agreement No 754658 (CARAMBA).

Cryopreservation in cryovials extends cell storage at low temperatures, and advances in organoid cryopreservation improve reproducibility and reduce generation time. However, cryopreserving human organoids presents challenges due to the limited diffusion of cryoprotective agents (CPAs) into the organoid core and the potential toxicity of these agents. To overcome these obstacles, we developed a cryopreservation technique using a pillar plate platform. To illustrate cryopreservation application to human brain organoids (HBOs), early-stage HBOs were produced by differentiating induced pluripotent stem cells (iPSCs) into neuroectoderm (NEs) in an ultralow atachement (ULA) 384-well plate. These NEs were transferred and encapsulated in Matrigel on the pillar plate. The early-stage HBOs on the pillar plate were exposed to four commercially available CPAs, including PSC cryopreservation kit, CryoStor CS10, 3dGRO, and 10% DMSO, before being frozen overnight at -80{degrees}C and subsequently stored in a liquid nitrogen dewar. We examined the impact of CPA type, organoid size, and CPA exposure duration on cell viability post-thaw. Additionally, the differentiation of early-stage HBOs on the pillar plate was assessed using RT-qPCR and immunofluorescence staining. The PSC cryopreservation kit proved to be the least toxic for preserving these HBOs on the pillar plate. Notably, smaller HBOs showed higher cell viability post-cryopreservation than larger ones. An incubation period of 80 minutes with the PSC kit was essential to ensure optimal CPA diffusion into HBOs with a diameter of 400 - 600 {micro}m. These cryopreserved early-stage HBOs successfully matured over 30 days, exhibiting gene expression patterns akin to non-cryopreserved HBOs. The cryopreserved early-stage HBOs on the pillar plate maintained high viability after thawing and successfully differentiated into mature HBOs. This on-chip cryopreservation method could extend to other small organoids, by integrating cryopreservation, thawing, culturing, staining, rinsing, and imaging processes within a single system, thereby preserving the 3D structure of the organoids.

With advancements in genetic diagnostics and genotype-based therapeutics, the demand for germline genetic testing in post-hematopoietic stem cell transplantation patients is increasing. Due to genetic chimerism, blood samples can no longer be used for germline testing after transplantation. This study aims to identify the most suitable tissue for germline analysis following stem cell transplantation by investigating alternative tissue sources. Buccal swab, eyebrow hair, and nail samples were analyzed for donor-derived DNA using next-generation sequencing and short tandem repeat analysis, with linear regression used for evaluation. Factors such as HLA match, transplantation type, sex, and time after transplantation were also evaluated for their effect on donor-derived DNA share. Buccal swab and nail samples exhibited 25% and 22% higher proportions of donor-derived DNA compared to eyebrow hair follicles, respectively. The median donor DNA share in eyebrow hair follicles was 1% for NGS and 3% for STR. Factors such as matched related donors, higher HLA match, different donor-recipient sex, and longer time post-transplantation correlated with lower donor DNA shares. Eyebrow hair follicles are a promising tissue for accurate germline genetic testing in post-SCT patients. Patient characteristics like donor relatedness, HLA match, sex match, and time after transplantation should be considered.