Small Methods

Spatial transcriptomics (ST) has emerged as a transformative tool for resolving the molecular heterogeneity of complex tissues within their native anatomical context. However, next-generation sequencing (NGS)-based ST platforms frequently encounter sensitivity bottlenecks arising from sub-optimal probe architectures on solid substrates. Conventional single-stranded DNA coupling methods often lead to disordered interfacial molecular conformations due to non-specific nucleobase-mediated surface tethering, which creates steric hindrance and inhibits the enzymatic efficiency of in situ library preparation. Here, we present Decomap (double-strand protected combinatorial barcoding microarray chip), a high-performance ST platform utilizing a triple-segment (dsZ-X-Y) fabrication strategy to achieve superior transcript capture efficiency. This structural optimization significantly enhances DNA ligation kinetics and subsequent polymerase-mediated extension, overcoming the fundamental limitations of traditional single-stranded coupling strategies. Decomap-seq achieved a median detection of 7,200 genes and 29,097 UMIs per 50 m-spot at a sequencing saturation of 50.1%. These results validate Decomap as a highly sensitive and robust tool for spatial transcriptomics, offering a powerful platform for advancing research in histopathology, developmental biology, and neuroscience.

Patient-derived tumor organoids (PDTOs) have emerged as valuable preclinical models for studying tumor biology and therapeutic responses. However, despite the development of protocols for tumor dissociation and immune cell infiltration, their fidelity in representing clear cell renal cell carcinoma (ccRCC) tumors remains poorly characterized. To address this, we established matched samples, including tumor tissue, enzymatically dissociated tumor, formed PDTOs, and immune-infiltrated PDTOs from three ccRCC patients, and performed bulk RNA sequencing to capture dynamic molecular changes across the experimental workflow. Our analyses revealed that tumor dissociation triggered stress-related transcriptional changes, marked by the upregulation of heat shock genes (e.g., HSPA1A) and the downregulation of the hypoxia pathway, while PDTOs recapitulated hypoxic signaling. Immune-infiltrated PDTOs retained critical immune signatures including T-effector, and exhibited an enhanced pro-inflammatory phenotype (CXCL10, JAK-STAT). Furthermore, predictive gene signatures and immunotherapy response scores further underscored the clinical relevance of immune-infiltrated PDTOs consistent with the original tumor tissue. Collectively, these findings validate immune-infiltrated PDTOs as robust, patient-specific models for personalized therapeutic exploration, offering a platform to optimize immunotherapy strategies in ccRCC.

Extracellular vesicles (EVs) are critical mediators of intercellular communication, carrying molecular cargos such as small noncoding RNAs (ncRNAs) that reflect the physiological and pathological state of their cells of origin. However, studying brain-derived EVs has been challenging due to the blood-brain barrier. Here, we optimized and validated an open-flow microdialysis (OFM) protocol for sampling EVs directly from brain interstitial fluid (ISF) in wild-type and APP/PS1 transgenic mice. Ex-vivo validation using plasma EVs demonstrated that OFM effectively captures the full EV population. In-vivo cerebral OFM (cOFM) enabled successful collection of brain ISF EVs, which were characterized by nanoparticle tracking analysis (NTA), electron microscopy, and western blotting, confirming their similarity to EVs isolated directly from brain tissue and plasma. Identification of small ncRNA cargos revealed that EVs sampled from brain ISF by cOFM were enriched in brain-specific signatures, many of which are associated with neuronal cell populations and biological functions. Furthermore, we observed a unique small ncRNA signature from the brain ISF EVs in the Alzheimers disease preclinical model compared to wild-type mice. These small ncRNAs were associated with genes considered important in biological functions associated with neurodegeneration. Our findings demonstrate that cOFM is a powerful tool for in-vivo sampling of brain EVs and highlight the unique molecular landscape of ISF EV small ncRNA cargos. This study offers new opportunities for biomarker discovery and mechanistic insights into neurodegenerative diseases, such as Alzheimers disease.

Cell mechanics can serve as an important biomarker for cell state and phenotype, such as metastatic ability. While some molecular mechanisms underlying cell mechanical properties have been investigated through targeted analyses, a genome-wide study of human genes and gene networks that modulate cell biophysical properties has not been attempted. In this work, we combined a microfluidic stiffness-based sorting device with a genome-scale CRISPR knockout (GeCKO) screen in order to investigate the effect of individual gene knockouts on cell stiffening and cell softening across the entire protein-coding genome. We processed approximately 150 million Cas9-expressing ovarian cancer cells that had been transduced with a library of 76,000 single guide RNAs (sgRNAs) against the 19,000 protein-coding genes in the genome. The cells were sorted into 5 mechanical subsets. We identified 7 gene knockouts that were significantly depleted in the softer subsets and over 700 gene knockouts that were significantly enriched in the stiffer subsets. Of these significant genes of interest, we selected 3 genes that were highly expressed in our ovarian cancer cell line with greater than 100-fold enrichment in the stiff outlet and resulted in significant changes in ovarian cancer patient survival. These genes, PIK3R4, CCDC88A, and GSK3B, when knocked out result in a significant and predicted increase in cell stiffness. This study is the first to explore the relation between human gene expression and cell mechanics at the genome-scale to generate datasets at the intersection between cell genotype, mechanotype, and phenotype for metastatic cancer cells. The method could also be applied to study the effect of genes on other biophysical cell processes as well as for identifying pathways for the control of cellular mechanics across many cell types.

Hematogenous metastasis is initiated when tumor cells (TCs) intravasate into the vasculature, yet intravasation remains poorly understood because it is difficult to observe in vivo and intravasated TCs are challenging to isolate. To address these challenges, we developed IntravChip, a continuously perfused microfluidic platform containing a vascularized primary tumor microenvironment (TME) enabling the observation of TC intravasation, and a downstream chamber to collect intravasated TCs. The IntravChip can support a high TC concentration in the TME while maintaining complete vascular perfusion, which we found was necessary to collect intravasated cells. Using MDA-MB-231 breast TCs, we identified an optimal initial TC seeding density that, by day 9, yields a densely populated TME and 100-440 collected intravasated TCs. We validated the IntravChip across several TC types, showing that MDA-MB-231 and MV3 TCs have the highest intravasation rates while MCF-7 TCs have low intravasation efficiency. We also show that the IntravChip is compatible with super-resolution nano-imaging. Our devices enabled high-quality STORM imaging, which revealed that H3K9me3 nanodomains are significantly differentially distributed in intravasated MDA-MB-231 tumor cells compared to those residing in the TME. Finally, the IntravChip was validated as a platform to test the effects of anti-cancer drugs on tumor cells and on the vasculature. We showed that a 5 M concentration of sorafenib reduced intravasation events by 69% without impacting the morphology of the microvascular networks (MVNs), while a 10 M concentration led to a significant decrease in vessel diameter. This platform enables quantitative analysis of TC intravasation, collection of intravasated TCs for characterization, and screening of anti-metastatic therapies.

Gel electrophoresis has been a cornerstone laboratory technique for decades, yet it is often viewed as cumbersome, costly, and has remained confined to laboratory settings. Recent advances in DNA nanotechnology have repurposed electrophoresis as a primary readout for some biosensing applications such as DNA nanoswitches, where a conformational change in a DNA structure indicates the presence of a target molecule. Conventional gel electrophoresis setups not ideal for such targeted applications, with moderate equipment cost, excessive reagent use, and time-consuming processes. Here, we adopt a reductionist, application-driven approach to redesign gel electrophoresis specifically for DNA nanoswitch-based detection. We present a fully 3D-printable mini gel electrophoresis system that incorporates conductive plastic electrodes, demonstrating performance comparable to conventional systems using platinum electrodes. By optimizing the inter-electrode distance and running parameters, our system resolves the on/off states of DNA nanoswitches in as little as one minute. We further show that the device operates reliably at low voltages, including when powered by a USB power bank, and even enables instrument-free nanoswitch readout using an LED with a cell-phone camera. Our design substantially reduces the cost, voltage requirements, material usage, operational complexity, and experiment time. These improvements make gel-based biosensing more practical outside traditional laboratory environments, paving the way for broader adoption of gel electrophoresis in point-of-care and resource-limited settings.

Precise characterization of regulatory sequence performance is fundamental to synthetic biology and next-generation gene therapies, driving the need for scalable and quantitative screening of genetic libraries. While droplet-based microfluidics offers the ultra-high throughput required to scale these assays, it often depends on complex, custom fluorescence-activated droplet sorting platforms. To address this limitation, we introduce an integrated microfluidic workflow that enables cell-free transcription in water-in-oil-in-water double emulsion picoreactors compatible with commercial flow cytometers. The core innovation is an integrated device that combines emulsion reinjection, electric-field-mediated step-injection of in vitro transcription (IVT) reagents, and downstream double emulsification, thereby reducing manual handling and preserving droplet integrity across multistep workflows. We validate the system by coupling isothermal rolling circle amplification (RCA) of DNA templates with on-chip IVT and Mango III aptamer-based fluorescence readout, demonstrating robust detection, binning, and sorting of transcription-active droplets. This workflow provides an accessible and modular platform for quantitative, high-throughput functional screening of regulatory sequences without the need for specialized optical sorting instrumentation.

Droplet sorting technology has the potential to revolutionize the biotechnology sector as it provides massive high-throughput screening capacity, but the technology remains not accessible for a wider audience yet. There is a need for more affordable droplet sorting platforms to design cell factories and screen cell libraries. In here we demonstrate our droplet cytometry/sorter platform for single-cell screening of yeast cells based on their fluorescence signal.

The superior stealth properties and high information density make DNA a sought-after candidate in the field of molecular steganography. Here, we developed the InfinMark end-to-end DNA steganography framework for anti-counterfeiting applications by combining the characteristics of both the Internet of Things (IoT) and DNA-of-Things (DoT). InfinMark includes five modules: Information Transcoding, Fingerprint Writing, Nano-encapsulation, Invisible Marking, and Multi-level Rapid Authentication. It ensures precise anti-counterfeiting information reading and writing through a dynamic DNA-compatible transcoding algorithm, achieves seamless embedding by developing scalable nanoparticle manufacture methods, and supports cross-scenario on-site verification, ultimately granting it comprehensive anti-counterfeiting capabilities spanning from source labeling to terminal tracing. By addressing the bottlenecks in IoT and DoT integration, lifecycle tracking, as well on-site product authentication, this research constructs a full-chain bimodal anti-counterfeiting system, thereby showcasing the practical application of informational DNA nanoparticles in various aspects of production and daily life.

Precise manipulation of gene expression is pivotal for gene function studies and the optimization of gene therapy. RNA-based gene switches are attractive tools due to their robust tunability by FDA-approved small molecules, the absence of exogenous immunogenic proteins, and the small size for gene delivery vectors such as adeno-associated virus (AAV). However, existing RNA switches only target a single step of gene expression such as transcription or RNA splicing, exhibiting intrinsic limitations in gene regulation. To overcome this issue, this study integrated the aptamer-based polyA regulator (pA), the drug-elicitable alternative splicing module (DreAM) and an engineered translation modulator with conditional upstream open reading frames (uORFs) to construct the DreAM-plus RNA switch. The pA-DreAM concatenation led to 1.5[~]5.0-fold and 1.2[~]4.4-fold increase of inducible fold changes than pA and DreAM, respectively. The uORF module further enhanced the switching performance by 1.4[~]6.3-fold. DreAM-plus-mediated transient transgene expression demonstrated a temporal resolution of about 24 hours and high tissue specificity to liver or heart. Critically, DreAM-plus achieved transient expression of an array of gene editors (SpCas9, SaCas9, Un1Cas12f1, OsCas12f1, AcCas12n, IsDra2 TnpB etc.) that significantly mitigated off-target effects by 1.4[~]2.8 folds in plasmids, lentivirus and AAV. In a new mouse model with lipid-nanoparticle-delivered pre-existing immunity, DreAM-plus attenuated AAV-delivered Cas-specific CD8 T cell immune toxicity in the liver and the heart. Therefore, multiple RNA switches could be synergistically integrated to build more sophisticated genetic cassettes for enhanced manipulation of gene expression.

Chromatin-associated RNAs play critical roles in regulating chromatin organization and transcription, underscoring the importance of their study. Proximity labeling has emerged as a promising and versatile technique for profiling chromatin-associated RNAs with high spatiotemporal resolution. While being a powerful technique, traditional proximity labeling methods depend on complex, high-input enrichment protocols, which significantly limit their wide practical application. Here, we developed a straightforward, enrichment-free chromatin-associated RNA profiling strategy: Proximity Crosslinking-induced RNA Depletion sequencing (PCRD-seq). This approach leverages the proximity crosslinking between chromatin and its surrounding RNAs induced by singlet oxygen generated by HoeDBF, a photosensitizer targeting chromatin region. The proximity crosslinking hinders the release of chromatin-associated RNAs during routine TRIzol extraction, consequently leading to a specific depletion of these RNAs. This method was successfully applied to investigate the role of U1 snRNA in RNA chromatin retention and the differences in chromatin-associated transcriptomes between two ovarian cancer cell lines with opposite metastatic capability. Moreover, our PCRD-seq exhibits potential in profiling nuclear lamina-associated RNAs, which paves the way for its application to profile RNAs associated with other chromatin subdomains. The minimal cell input and simple workflow endow PCRD-seq as a transformative tool for wide applications.

Efficient, aggregation-free extracellular vesicles (EVs) labeling is essential for studying their dynamics in-vitro and in-vivo. However, traditional dyes introduce limitations including aggregation, membrane intercalation, fluorescence transfer and inconsistent performance across EV sources thus distorting quantification, altering surface properties and confounding uptake and biodistribution analyses. Here, we systematically evaluated CytoLight, a luminal dye traditionally used for live-cell imaging, as an alternative for EV quantification, characterization, uptake analysis and in-vivo tracking, benchmarking it against PKH26, CFSE and ExoBrite across multiple platforms. CytoLight generated stable, intravesicular fluorescence without aggregation or membrane alteration, eliminating artifacts characteristic of conventional dyes. Using fluorescence-NTA and single-EV flow cytometry, CytoLight showed more consistent labeling across EV types than CFSE or ExoBrite, while avoiding PKH-related micelle-driven artifacts and exhibited compatibility with CD81 dual-detection. In uptake assays, CytoLight produced EV-specific endocytosis-dependent internalization signals exceeding labeled-BPS/protein controls. In-vivo, CytoLight-labeled EVs enabled fluorescent biodistribution mapping showing conventional EV tropism patterns distinguishable from labeled-PBS controls. These findings establish CytoLight as an effective, aggregation-free EV-labeling strategy. Its stability, specificity, compatibility with single-EV platforms and reliable performance in both cellular uptake and biodistribution studies position CytoLight as a practical, scalable alternative to current dyes, providing a stronger foundation for standardized and reproducible EV research.

Cerebral blood volume (CBV) and blood flow (CBF) constitute key metrics for cerebrovascular monitoring, enabling assessment of stroke severity and risk-prediction, aging-related changes, and neurological diseases. CBF and CBV monitoring are key aspects in diagnosis, treatment triage, and clinical outcome of ischemic and hemorrhagic strokes. In recent years, there have been ongoing efforts toward the development of optical devices for noninvasive monitoring of CBV and CBF. Speckle contrast optical spectroscopy (SCOS) has recently emerged as a strong candidate for clinical translation in monitoring CBF and CBV, due to its affordability, compact and wearable design, and noninvasive nature. However, experimental demonstrations that SCOS can effectively monitor brain hemodynamics remain sparse. This is primarily due to challenges in design experiments that isolate cerebral blood dynamics from those in the scalp and skull. In this paper, we report experiments using SCOS to monitor cerebral hemodynamics in rats during intracerebral blood flow modulation. To modify cerebral blood dynamics, a surgical procedure was performed to insert a catheter for direct injection of flow modulation fluids into the brain. Using the SCOS device, we monitored changes in CBV during deliberate CBF interventions into the brains of five rats. A saline solution was also injected as a sham control of the flow intervention. The results show a significant decrease in CBV during injection, followed by a return to baseline. This behavior is consistent with physiological expectations, as the injected fluids dilute the blood, leading to a transient reduction in blood volume. Notably, the CBV decrease induced by the flow modulation fluid solution required more than twice as long to recover to baseline compared with the saline solution, which is consistent with the delayed clearance of the flow modulation fluid by design. These experimental results demonstrate the effectiveness of SCOS for monitoring cerebral hemodynamics in animal models and highlight its potential for translation to human studies. Moreover, this work paves the way for the testing and characterization of cerebral therapeutic agents intended for blood flow modulation in animal models.

Understanding biophysical phenomena requires techniques that access biologically relevant spatial and temporal scales. Expansion Microscopy (ExM) is a sample preparation approach which achieves super-resolution spatial scales by leveraging osmotic forces in a swellable hydrogel to physically separate structures to distances larger than the diffraction limit of light. Yet, in traditional osmotic ExM only pre- and post- expanded samples can be imaged. Further, fragmentation, hydrogel deformation, and signal loss are common while requiring samples to be chemically fixed. Therefore, there is little control of the expansion, reproducibility can be challenging, and dynamics of biological samples at applicable temporal scales cannot be observed. Here, we develop Tensile Expansion Microscopy (TExM) to mechanically expand fixed and, notably, living cellular samples. Highly-stretchable and tough double network alginate- Ca2+/polyacrylamide hydrogels are expanded by tensile forces applied using an electromechanical iris expansion device during continuous imaging on a fluorescence microscope. We incorporate two-photon polymerized microscale fluorescent fiducial markers to track samples and distortion during expansion. The hydrogels controllably and repeatedly expand up to 3.3x with distortions less than 12 {micro}m across 1.3 mm2. TExM is first applied to fixed NIH 3T3 fibroblast cells with immunohistochemistry-stained microtubules, achieving super-resolutions of 100 nm. Then, TExM is demonstrated with living HeLa cells with internal fluorescent reporters showing increased cell size and cell-to-cell separation under 3.2x linear expansion. Overall, TExM allows for continuous, stepwise, and precise temporal modulation of lateral substrate strain, enabling real time monitoring of dynamics of both fixed and viable live cell processes at higher spatial resolutions. TExM can further investigate broad biophysical questions due to its compatibility with other analytical imaging methods that are sensitive to water or fixatives used in traditional osmotic ExM.

Many experiments rely on expensive or scarce liquids, such as costly reagents, or biological samples available only in limited quantities. Droplet microarrays are an especially promising approach to conserving these materials because they support highly parallelized reactions in small volumes. However, existing droplet microarray loading methods based on discontinuous dewetting suffer from loading inconsistencies and large dead volumes. In this work, we present the Small Volume Loader (SVL) for the Surface Patterned Omniphobic Tiles (SPOTs) platform that enables precise deposition on droplet microarrays while minimizing reagent waste. By establishing a physical model of the loading process, we identified that deposition volume is governed by the sum of hydrostatic and Laplace pressures at the reservoir outlet. To optimize performance, we engineered a pressure-compensating flared reservoir geometry that maintains constant total pressure regardless of the remaining liquid level. This design ensures that the deposited volume is independent of reservoir volume and reduces dead volume to 5 L. We demonstrated the platforms utility through high-throughput elicitor screening for natural antimicrobial production from Streptomyces venezuelae. The resulting assays used 100-fold less material than conventional methods, allowing us to conduct over 32,000 assays with modest quantities of starting material. This enabled us to identify specific stressors that optimize the production of the antibiotics chloramphenicol and jadomycin B. Together, we demonstrated improved loading performance for droplet microarray platforms, allowing precise, accessible, and high-throughput assays using only minimal volumes of scarce materials.

A critical challenge in endocrine neurosurgery is intraoperative discrimination between normal pituitary tissue and pituitary neuroendocrine tumors (PitNETs). Suggesting the universal persistence of near-infrared autofluorescence (NIRAF) in endocrine organs and inspired by routine clinical use of NIRAF for parathyroid gland identification, we discovered that pituitary NIRAF can be employed for label-free transsphenoidal surgery guidance. Ex vivo confocal spectral imaging of 33 specimens identified secretory granules as the dominant long-wavelength fluorescence source and showed that normal pituitary had higher granule content than PitNETs. For the first time, we made use of the pituitary NIRAF during surgery and assessed its performance for pituitary/adenoma separation in vivo for 27 surgeries and showed near-perfect separability between pituitary and non-pituitary measurement sites with ROC-AUC of 0.98. The obtained results clearly demonstrate that the suggested method, based on the solid microscopic background, has the potential for clinical translation and paves the way for enhanced gland preservation during resection.

Cellular immunotherapy has revolutionized cancer treatment by enabling more targeted and personalized disease management. As the field progresses, there is an increasing need for high-throughput in vitro assays to efficiently assess the cytotoxicity of therapeutic cells. Conventional cytotoxicity assays pose various limitations in the workflow and scalability. Here, we present an mRNA lipid nanoparticle (mRNA-LNP) approach to efficiently and robustly deliver reporter genes to target cells for assessing immune effector cell-mediated cytotoxicity. This approach enables the rapid, homogenous reporter expression without compromising the viability of target cells. The cytotoxicity results obtained using mRNA-LNP-transfected cells are highly consistent and comparable to those obtained using cell lines with stable reporter gene expression. Finally, we highlight the mRNA-LNP approachs compatibility across a diverse range of tumor models, including primary tumor-derived models, enabling rapid and high-throughput assessment of the potency of various cytotoxic therapeutic cells.

siRNA delivery platforms capable of accessing both central and peripheral tissues are critically needed to expand the therapeutic potential of oligonucleotides. To address this, we developed a novel siRNA-antibody conjugate by attaching an Hprt-targeting siRNA to an engineered antibody shuttle. This shuttle targets the insulin-like growth factor 1 receptor (IGF1R) using a fused antibody fragment (Clone F) and utilizes an antibody backbone with no tissue-relevant binding in this study. The resulting conjugate, designated Clone F-Hprt, demonstrated robust in vivo knockdown across multiple tissues. Clone F-Hprt demonstrated enhanced penetration into central nervous system (CNS) tissues compared to unconjugated siRNA following intracerebroventricular (ICV) and intravenous (IV) administration. In peripheral tissues, Clone F-Hprt achieved widespread knockdown in muscle, heart, and lung, consistent with IGF1R expression. The conjugate was well tolerated across all routes, including with repeated dosing. Although several receptor-mediated approaches for CNS delivery are progressing to the clinic (e.g., targeting the transferrin receptor), clinical validation remains to be demonstrated. Our findings highlight IGF1R as an alternative receptor capable of supporting delivery across both central and peripheral tissues, offering a complementary strategy for expanding the therapeutic landscape of oligonucleotide delivery.

Receptor tyrosine kinase signaling is initiated by extracellular ligand binding, which drives the formation of membrane-protein assemblies that activate intracellular signal transduction. Accurately resolving the molecular composition of these assemblies in situ remains challenging due to their nanoscale dimensions and intrinsic heterogeneity. Here, we introduce a single-molecule super-resolution imaging and analysis workflow designed to resolve and quantitatively characterize individual membrane-protein assembly sites in cells. We apply this approach to the nanoscale organization of the epidermal growth factor receptor (EGFR) and its adaptor protein Grb2 following stimulation with the native ligand epidermal growth factor (EGF). As activation progresses, we observe a reduction in EGFR density at the plasma membrane, a progressive accumulation of Grb2 at EGFR assembly sites, and an increase in both dimeric and higher-order oligomeric EGFR. The experimental and analytical framework presented here is broadly applicable to the study of diverse membrane-protein assemblies.

Extracellular vesicles (EVs) carry molecular cargo that can reflect the real-time state of parental cells, yet most in vitro EV analyses rely on bulk approaches and therefore average over pronounced heterogeneity in both cell and EV populations. Here, we present a semi-open microfluidic platform that enables multi-marker profiling of EVs released from single-cell-derived clones, allowing EV signatures to be linked to clonal progeny originating from a single parental cell. The platform integrates aligned cell and EV arrays containing 17,305 wells, assembled with a 3D-printed housing to capture released EVs in one-to-one matched wells. Captured EVs are immunolabeled for canonical tetraspanin markers (CD9, CD63, CD81) and EpCAM, imaged by high-resolution fluorescence microscopy, and quantified using an automated image-analysis pipeline. Applying the platform to single-cell-derived PC3 clones revealed substantial heterogeneity in EV marker co-expression, with hierarchical clustering identifying four distinct tetraspanin co-expression profiles. The fraction of EpCAM-positive EVs increased with PC3 cell proliferation, as assessed by endpoint cell number, whereas free (non-EV-associated) EpCAM showed no correlation. This platform enables near single-EV-level, multi-marker profiling from single-cell lineages and provides a practical approach to simultaneously dissect both cellular and EV heterogeneity.