CD8 Antibody, FITC

What is CD8 and why is it an important target for immunological research?

CD8 is a type I transmembrane glycoprotein of the immunoglobulin family that plays an integral role in signal transduction, T cell differentiation, and activation. It exists on the cell surface primarily as either a disulfide-linked heterodimer (CD8αβ) or homodimer (CD8αα). The CD8α chain is essential for binding to MHC class I molecules, where it functions as a co-receptor alongside the T cell receptor (TCR) . CD8 is predominantly expressed on cytotoxic T lymphocytes (CTLs), certain subpopulations of αβ T cells and γδ T cells, and some NK cells .

The importance of CD8 in research stems from its critical role in the adaptive immune response. When activated through ligation of MHC-I/peptide complexes presented by antigen-presenting cells, CD8+ T cells trigger recruitment of lymphocyte-specific protein tyrosine kinase (Lck), leading to lymphokine production, motility, and CTL activation . These activated CTLs are crucial for clearing pathogens and tumor cells, making CD8 an essential marker for studying immune responses to infections and cancer .

What makes FITC a suitable fluorochrome for CD8 antibody conjugation?

FITC (Fluorescein Isothiocyanate) is one of the most widely used fluorochromes for antibody conjugation due to several advantageous properties. It provides relatively high absorptivity, excellent fluorescence quantum yield, and good water solubility . These characteristics make FITC-conjugated antibodies reliable tools for flow cytometry applications.

How do different CD8 antibody clones (3B5, HIT8a, MEM-31, EP72) differ in their applications?

Different CD8 antibody clones recognize distinct epitopes of the CD8 molecule, which affects their applications and performance:

• Clone 3B5: This monoclonal antibody targets CD8 and is commonly used for flow cytometry applications. It recognizes CD8α and is suitable for identifying CD8+ T lymphocytes in research settings .

• Clone HIT8a: This clone specifically binds to CD8α and is noted for not cross-blocking with other clones like RPA-T8. This characteristic makes it valuable for co-staining experiments where multiple CD8 epitopes need to be detected simultaneously .

• Clone MEM-31: This antibody recognizes a conformationally-dependent extracellular epitope of CD8. Importantly, it does not react with formaldehyde-fixed cells and is negative in Western blotting applications. This makes it specifically suitable for flow cytometry applications with fresh or appropriately preserved samples .

• Clone EP72: This monoclonal antibody has been validated for flow cytometry and immunohistochemistry on frozen sections (IHC-Fr), particularly with chicken samples. Its specific binding properties make it suitable for these particular applications and species .

When selecting a clone, researchers should consider the specific application, sample preparation method, and epitope accessibility in their experimental conditions.

What are the standard protocols for using CD8-FITC antibodies in flow cytometry?

When using CD8-FITC antibodies for flow cytometry, researchers should follow these methodological steps:

• Sample Preparation:

  • Isolate cells from your tissue of interest using appropriate methods (e.g., density gradient separation for PBMCs)

  • Wash cells in flow cytometry buffer (PBS with 1-2% serum and 0.1% sodium azide)

  • Adjust cell concentration to approximately 1 × 10^6 cells per 100 μl test volume

• Staining Protocol:

  • Use pre-diluted antibodies at the recommended volume per test

  • Include appropriate isotype controls at the same concentration as your antibody of interest

  • For surface staining, incubate cells with CD8-FITC antibody for 20-30 minutes at 4°C in the dark

  • Wash cells 2-3 times with flow cytometry buffer to remove unbound antibody

  • If performing multi-color analysis, consider compensation controls to address spectral overlap

• Instrument Setup and Analysis:

  • Configure your flow cytometer according to the fluorochrome spectra

  • Use proper compensation settings if multiple fluorochromes are employed

  • Analyze your data using appropriate gating strategies to identify CD8+ populations

• Quality Control Considerations:

  • Include viability dyes to exclude dead cells

  • Use FMO (fluorescence minus one) controls when establishing complex panels

  • Consider the expression level of CD8 when interpreting results—CD8 is typically highly expressed on cytotoxic T cells but may vary in different cell subsets or activation states

Remember that antibody performance can vary between lots and manufacturers, so validation with appropriate controls is essential before conducting critical experiments.

How can CD8-FITC antibodies be effectively incorporated into multi-parameter flow cytometry panels?

Incorporating CD8-FITC antibodies into multi-parameter flow cytometry requires careful panel design that considers marker expression levels, fluorochrome brightness, and potential spectral overlap. A systematic approach involves:

• Marker Prioritization Using the Tier System:

  • CD8 typically falls into the primary tier of phenotypic markers used for basic cell identification

  • Secondary tier markers might include activation and exhaustion markers

  • Tertiary tier markers, which are often your experimental variables with lower expression, should be paired with the brightest fluorochromes

• Strategic Fluorochrome Selection:

  • Since CD8 is usually highly expressed, FITC is generally suitable despite its moderate brightness

  • Reserve brighter fluorochromes (PE, APC, PE-Cy7) for markers with lower expression levels

  • Consider the specific optical configuration of your flow cytometer to optimize detection sensitivity

• Managing Spectral Overlap:

  • FITC emission overlaps primarily with PE, so plan your panel accordingly

  • When using FITC with other green-yellow fluorochromes, ensure proper compensation controls

  • Single-stained controls should be prepared for each fluorochrome in your panel

• Panel Validation Strategy:

  • Test the full panel on control samples before proceeding to valuable research samples

  • Evaluate potential fluorescence spread and adjust the panel if certain markers show significant interference

  • Compare the performance of markers when stained individually versus in the full panel

For example, when studying CD8+ T cell exhaustion, a panel might include:

• CD8-FITC (primary tier)

• CD3-APC (primary tier)

• PD-1-PE (secondary tier, activation/exhaustion)

• CD57-BV421 (secondary tier, senescence marker)

• CD137-PE-Cy7 (tertiary tier, activation marker for tumor-reactive T cells)

This approach ensures optimal detection of all markers while minimizing interference between fluorochromes.

What are the key considerations when using CD8-FITC antibodies to identify and characterize different CD8+ T cell subsets?

Identifying and characterizing distinct CD8+ T cell subsets requires thoughtful experimental design and interpretation of CD8-FITC antibody staining in conjunction with other markers. Key considerations include:

• Differential Expression Patterns:

  • CD8 exists as both αα homodimers and αβ heterodimers, with different distributions across T cell subsets

  • CD8αβ heterodimers are predominantly found on conventional αβ T cells, while some γδ T cells and NK cells express CD8αα homodimers

  • Consider using antibodies that can distinguish between these forms if relevant to your research question

• Subset-Defining Marker Combinations:

  • Differentiation states: CD8+ T cells can be classified as early-differentiated (CD27+CD8+CD57−), intermediate-differentiated (CD27+CD8+CD57+), and terminally-differentiated (CD27−CD8+CD57+)

  • Functional phenotypes: Additional markers like FOXP3 can identify regulatory CD8+ T cells, with CD57−FOXP3+CD8+ and CD57+FOXP3+CD8+ T cells showing different prognostic associations

  • Activation/exhaustion states: Markers such as PD-1, CD39, CD160, TIM-3, TIGIT, and TOX help identify activated and exhausted-like CD8+ T cells

• Functional Correlation:

  • Terminally-differentiated CD27−CD8+CD57+ T cells are typically GBhighperforinhigh (highly cytotoxic)

  • Incompletely differentiated CD27+CD8+CD57+ T cells are typically GB+perforin−/low (poorly cytotoxic)

  • Consider including functional assays to validate the phenotypic characterization

• Context-Specific Interpretations:

  • CD137+ expression identifies tumor-reactive CD8+ T cells with an activated and exhausted-like phenotype that show superior anti-cancer activity in adoptive transfer models

  • The same phenotypic markers may have different implications depending on the disease context (cancer, chronic infection, autoimmunity)

This multi-dimensional approach allows for more precise identification of functionally relevant CD8+ T cell populations beyond what a single CD8-FITC staining could provide.

How can researchers address potential artifacts or limitations when using CD8-FITC antibodies in flow cytometry experiments?

Several artifacts and limitations may affect the interpretation of CD8-FITC antibody staining in flow cytometry. Addressing these requires methodological rigor:

• Autofluorescence Management:

  • FITC emission overlaps with the autofluorescence spectrum of many cell types, particularly activated or aged cells

  • Methodological solution: Include unstained controls for each sample type and consider using spectral flow cytometry with autofluorescence extraction algorithms

  • For tissues with high autofluorescence, consider alternative fluorochromes with emission in different spectral regions

• Epitope Masking and Accessibility Issues:

  • Some CD8 antibody clones (e.g., MEM-31) recognize conformationally-dependent epitopes that may be affected by fixation procedures

  • Methodological solution: Optimize fixation protocols or select clones known to work with your fixation method

  • For intracellular staining protocols, verify that the CD8 epitope remains accessible after permeabilization

• Spectral Compensation Challenges:

  • FITC compensation can be particularly challenging when used alongside PE or other green-yellow fluorochromes

  • Methodological solution: Use single-stained controls for each fluorochrome on the same cell type as your experimental samples

  • Consider computational approaches like automated compensation algorithms for complex panels

• Antibody Internalization During Processing:

  • CD8 receptors can be internalized upon activation or during certain processing steps

  • Methodological solution: Minimize processing time, maintain samples at 4°C, and consider kinetic studies to understand potential internalization effects

  • For activated cells, comparing CD8 surface expression over time can help interpret apparent changes in staining intensity

• Clone-Specific Limitations:

  • Different CD8 antibody clones have specific binding characteristics and limitations

  • Methodological solution: Select clones based on your specific application and validate with appropriate controls

  • For example, avoid using MEM-31 for fixed samples or Western blotting applications

By anticipating these potential issues and implementing appropriate controls and optimization steps, researchers can enhance the reliability of their CD8-FITC flow cytometry data.

What are the current advanced applications of CD8-FITC antibodies in tumor immunology research?

CD8-FITC antibodies have become integral tools in cutting-edge tumor immunology research, with several advanced applications:

• Identification of Tumor-Reactive CD8+ T Cell Populations:

  • CD137+ (4-1BB) expression on CD8+ T cells helps identify tumor-reactive populations with superior anti-cancer activity

  • Methodology: Multi-parameter flow cytometry combining CD8-FITC with markers like CD137, PD-1, CD39, and other exhaustion markers enables identification of these specialized cells

  • These CD137+CD8+ T cells display a highly proliferative, fully activated effector and exhausted-like phenotype with enhanced expression of PD-1, CD39, CD160, TIM-3, TIGIT, TOX, and CD57

• Prognostic Assessment of CD8+ T Cell Phenotypes:

  • Different CD8+ T cell phenotypes correlate with disease outcomes in cancer patients

  • Terminally-differentiated CD8+ T cells (CD27−CD8+CD57+) associate with longer progression-free survival in some cancers

  • Conversely, CD57−FOXP3+CD8+ T cells correlate with shorter progression-free survival and represent an independent poor prognostic factor

  • Methodology: Flow cytometric or immunohistochemical analysis of tumor-infiltrating lymphocytes using CD8-FITC combined with differentiation and regulatory markers

• Adoptive Cell Therapy Development:

  • CD8-FITC antibodies help isolate and characterize CD8+ T cell populations for adoptive transfer

  • CD137+CD8+ T cells have demonstrated superior anti-cancer activity in humanized mouse models

  • Methodology: Flow cytometry-assisted cell sorting using CD8-FITC along with activation markers enables isolation of specific subsets for expansion and therapeutic use

  • Mice receiving adoptively transferred CD137+CD8+ T cells showed reduced tumor growth and higher CD8+ T cell tumor infiltration compared to those receiving CD137−PD-1−CD8+ T cells or bulk CD8+ T cells

• Humanized Mouse Model Development:

  • CD8-FITC antibodies facilitate tracking of human CD8+ T cell responses in humanized mouse models

  • These models provide tools for immunotherapy research by enabling the study of human T cell subsets like activated and exhausted-like effector CD8+ T cells

  • Methodology: Flow cytometric analysis of human CD8+ T cell differentiation into phenotypes like terminal exhausted (Tex-term) and tissue-resident (TRM) cells in tumor-bearing humanized mice

These advanced applications demonstrate how CD8-FITC antibodies contribute to our understanding of tumor immunology and the development of novel immunotherapeutic approaches.

How can researchers optimize staining protocols when CD8-FITC antibodies show weak signal or high background?

Optimizing CD8-FITC antibody staining requires systematic troubleshooting of several variables:

• For Weak Signal Issues:

  • Antibody Titration: Perform a titration series (e.g., 1:50, 1:100, 1:200, 1:400) to identify the optimal concentration that maximizes signal-to-noise ratio

  • Incubation Conditions: Extend incubation time to 45-60 minutes at 4°C in the dark to enhance binding while minimizing internalization

  • Buffer Optimization: Use high-quality flow cytometry buffer with freshly added protein (2% BSA or FBS) to prevent non-specific binding while maintaining epitope accessibility

  • Sample Handling: Minimize processing time, maintain sample viability, and avoid repeated freeze-thaw cycles of antibodies

  • Clone Selection: Test alternative CD8 antibody clones if epitope accessibility might be an issue with your current clone

• For High Background Issues:

  • Fc Receptor Blocking: Pre-block samples with Fc receptor blocking reagents (10-15 minutes before antibody addition)

  • Washing Protocol: Implement more stringent washing (3-4 washes with larger volumes) to remove unbound antibody

  • Viability Dye: Include a viability dye to exclude dead cells, which often exhibit high autofluorescence and non-specific binding

  • Filtration: Filter samples through a 35-70μm mesh before acquisition to remove aggregates

  • Compensation Adjustment: Carefully review and adjust compensation settings, as FITC spectral overlap can contribute to apparent high background in other channels

• Instrument-Related Optimization:

  • PMT Voltage: Adjust photomultiplier tube voltage for optimal detection of FITC signal

  • Threshold Settings: Optimize threshold settings to exclude debris while capturing all cells of interest

  • Regular Calibration: Ensure regular calibration of the flow cytometer using standardized beads

• Sample-Specific Considerations:

  • Autofluorescence Reduction: For highly autofluorescent samples (like lung or skin cells), consider autofluorescence quenching reagents

  • Alternative Fluorochromes: In cases of persistent autofluorescence issues, consider switching from FITC to fluorochromes with different spectral properties

By systematically addressing these variables, researchers can significantly improve CD8-FITC antibody staining quality and reliability.

What controls should be included when using CD8-FITC antibodies in multi-parameter flow cytometry?

A comprehensive control strategy is essential for reliable interpretation of CD8-FITC antibody staining in multi-parameter flow cytometry:

• Essential Control Types:

  • Isotype Controls: Include a FITC-conjugated isotype-matched control antibody at the same concentration as the CD8-FITC antibody to assess non-specific binding

  • Unstained Controls: Prepare samples with no antibodies to establish baseline autofluorescence

  • Single-Stained Controls: For each fluorochrome in your panel, prepare a single-stained sample for compensation setup

  • Fluorescence Minus One (FMO) Controls: Include controls where each sample contains all fluorochromes except one to accurately set gating boundaries, especially for markers with continuous expression patterns

• Biological Controls:

  • Positive Control Samples: Include samples known to contain CD8+ cells (e.g., peripheral blood lymphocytes) to confirm antibody functionality

  • Negative Control Samples: Use cell types known not to express CD8 (e.g., CD4+ sorted T cells) to verify specificity

  • Blocking Controls: For verification of specificity, include samples pre-blocked with unconjugated CD8 antibody before adding CD8-FITC

• Quality Control Measures:

  • Viability Discrimination: Include a viability dye to exclude dead cells, which often exhibit altered marker expression and increased non-specific binding

  • Doublet Exclusion: Implement FSC-H vs. FSC-A or similar gating strategies to exclude cell doublets that can confound results

  • Time Parameter Monitoring: Record time during acquisition to identify potential flow interruptions or instrument issues

• Standardization Controls:

  • Antibody Capture Beads: Use anti-mouse Ig beads labeled with CD8-FITC for consistent instrument setup across experiments

  • Reference Standards: Include stabilized control cells or commercial control samples when available for longitudinal consistency

  • Internal Controls: When applicable, include spike-in control cells with known CD8 expression levels to normalize across batches

This comprehensive control strategy allows for accurate data interpretation and troubleshooting of potential issues with CD8-FITC antibody staining.

How do fixation and permeabilization protocols affect CD8-FITC antibody performance in flow cytometry?

Fixation and permeabilization can significantly impact CD8-FITC antibody staining characteristics, requiring careful protocol selection:

• Effects of Different Fixation Methods:

  • Paraformaldehyde (PFA)/Formaldehyde:

    • Mild fixation (0.5-2% PFA) generally preserves CD8 epitopes recognized by most clones

    • Extended fixation times or higher concentrations may reduce staining intensity

    • Some clones (e.g., MEM-31) specifically do not work with formaldehyde-fixed cells

  • Alcohol-Based Fixatives:

    • Methanol or ethanol fixation can denature certain CD8 epitopes

    • May be unsuitable for certain CD8 antibody clones that recognize conformational epitopes

    • Often used for intracellular staining protocols, requiring verification of compatible CD8 antibody clones

• Sequential Staining Strategies:

  • Surface-First Approach:

    • Stain with CD8-FITC before fixation/permeabilization to preserve epitope recognition

    • Verify FITC fluorescence stability through your specific fixation protocol

    • May require higher initial antibody concentration to account for potential signal loss

  • Post-Fixation Staining:

    • Some epitopes remain accessible after fixation but before permeabilization

    • Test different fixatives and concentrations to determine optimal conditions for your specific CD8-FITC antibody clone

• Protocol-Specific Considerations:

  • Intracellular Cytokine Staining:

    • CD8 surface staining should generally precede fixation/permeabilization

    • Brief fixation (10-15 minutes with 2-4% PFA) typically maintains CD8-FITC signal

    • Commercial fixation/permeabilization kits often provide optimized protocols for maintaining surface marker detection

  • Transcription Factor Staining:

    • Harsher fixation/permeabilization required for nuclear antigens may diminish CD8-FITC signal

    • Consider using brighter fluorochromes for CD8 if performing transcription factor analysis (e.g., of FOXP3 in CD8+ regulatory T cells)

• Methodological Solutions:

  • Antibody Cocktail Optimization:

    • For multi-step protocols, determine whether CD8-FITC performs better in pre- or post-fixation cocktails

    • Some protocols may benefit from restaining surface markers after fixation/permeabilization

  • Clone Selection Based on Protocol:

    • Select CD8 antibody clones documented to work with your specific fixation/permeabilization method

    • Avoid clone MEM-31 for any protocols requiring formaldehyde fixation

By understanding these interactions and testing protocols systematically, researchers can optimize CD8-FITC antibody performance in experiments requiring fixation and permeabilization.

What are the best practices for analyzing CD8+ T cell subpopulations with varying CD8 expression levels?

Analyzing CD8+ T cell subpopulations with heterogeneous CD8 expression requires sophisticated approaches:

• Gating Strategies for Variable Expression:

  • Biexponential Display: Use biexponential scaling rather than logarithmic scaling to better visualize the full range of CD8 expression

  • Contour Plots: Employ contour plots with percentage gating to identify populations that might be obscured in dot plots

  • Density-Based Clustering: Consider computational approaches like t-SNE or UMAP for unbiased identification of populations with subtle differences in CD8 expression

• Resolving CD8dim Populations:

  • Additional Markers: Incorporate lineage-specific markers to confirm the identity of CD8dim populations

  • Back-Gating Analysis: After identifying cell populations based on other markers, back-gate onto CD8 expression to characterize CD8 levels in different functional subsets

  • Reference Populations: Use internal reference populations with stable CD8 expression to normalize and interpret CD8dim signals

• Multi-Parameter Analysis Approaches:

  • Co-expression Patterns: Analyze CD8 expression in conjunction with markers of differentiation states (CD27, CD57) or activation (CD137)

  • Boolean Gating: Create combinatorial gates to identify complex phenotypes like CD27−CD8+CD57+ (terminally differentiated) versus CD27+CD8+CD57− (early differentiated) T cells

  • Hierarchical Gating: Implement a hierarchical gating strategy starting with lineage markers before examining CD8 expression levels

• Quantitative Assessment Methods:

  • Mean Fluorescence Intensity (MFI): Report CD8 expression levels as MFI for different subpopulations to quantify expression differences

  • Molecules of Equivalent Soluble Fluorochrome (MESF): Convert fluorescence intensity to standardized MESF values for more precise quantification across experiments

  • Receptor Occupancy Calculation: For certain applications, calculate the percentage of occupied CD8 receptors using saturating concentrations of antibodies

• Context-Specific Interpretation:

  • Activation-Induced Modulation: Account for CD8 downregulation upon T cell activation when interpreting reduced CD8 staining

  • Tissue-Specific Variations: Recognize that CD8 expression levels may vary between blood, lymphoid tissues, and tissue-resident populations

  • Species Differences: Consider species-specific patterns of CD8 expression when working with models beyond human samples

By implementing these best practices, researchers can accurately identify and characterize CD8+ T cell subpopulations despite variations in CD8 expression levels.

How are advancements in flow cytometry technology changing the applications of CD8-FITC antibodies in research?

Technological advancements in flow cytometry are expanding the applications and enhancing the utility of CD8-FITC antibodies in several ways:

• Spectral Flow Cytometry Advancements:

  • Full spectrum analysis allows better resolution of FITC signal from autofluorescence, improving the signal-to-noise ratio

  • Unmixing algorithms can separate FITC signal from spectrally adjacent fluorochromes more effectively

  • These advances enable more complex panels incorporating CD8-FITC alongside fluorochromes that would traditionally show significant spectral overlap

• Single-Cell Multiomics Integration:

  • Flow cytometry index sorting with CD8-FITC can be paired with single-cell RNA sequencing to correlate protein expression with transcriptional profiles

  • CITE-seq and similar technologies allow simultaneous detection of CD8 protein expression and mRNA transcripts

  • These integrated approaches provide deeper insights into the functional heterogeneity of CD8+ T cell populations

• High-Dimensional Data Analysis Tools:

  • Machine learning algorithms can identify novel CD8+ T cell subsets based on complex marker combinations that include CD8-FITC

  • Dimensionality reduction techniques like t-SNE, UMAP, and FlowSOM facilitate visualization and interpretation of high-parameter data

  • These computational approaches are particularly valuable for identifying functionally distinct CD8+ T cell populations like tumor-reactive CD137+CD8+ T cells

• Imaging Flow Cytometry Applications:

  • Combines traditional flow cytometry with microscopy to provide morphological information alongside CD8-FITC fluorescence data

  • Enables assessment of CD8 receptor localization, clustering, or internalization in different functional states

  • Particularly valuable for studying immunological synapse formation in CD8+ T cells

• Translational Research Applications:

  • More sensitive detection systems enable better identification of rare CD8+ T cell populations with clinical significance

  • Standardization efforts improve inter-laboratory reproducibility, facilitating multi-center clinical studies

  • These advances support the development of CD8+ T cell-based cellular therapies, such as those leveraging the superior anti-cancer activity of CD137+CD8+ T cells

As flow cytometry technology continues to evolve, researchers can expect improved sensitivity, greater panel complexity, and enhanced integration with other technologies when using CD8-FITC antibodies, ultimately advancing our understanding of CD8+ T cell biology in health and disease.

What future directions are emerging for CD8-FITC antibody applications in immunotherapy research?

Emerging trends suggest several promising future directions for CD8-FITC antibody applications in immunotherapy research:

• Precision Immunophenotyping for Personalized Immunotherapy:

  • High-dimensional phenotyping using CD8-FITC alongside markers of activation, exhaustion, and tumor reactivity (e.g., CD137)

  • Correlation of CD8+ T cell phenotypes with treatment outcomes to identify predictive biomarkers

  • Development of patient-specific immunotherapy strategies based on CD8+ T cell subset analysis

• Advanced Adoptive Cell Therapy Applications:

  • Isolation and expansion of specific CD8+ T cell subsets with superior anti-cancer activity, such as CD137+CD8+ T cells

  • Real-time monitoring of adoptively transferred CD8+ T cells to assess persistence, function, and tumor infiltration

  • Engineering of CD8+ T cells with enhanced functionality based on insights from comprehensive phenotyping

• Tissue-Resident Memory T Cell Research:

  • Characterization of tissue-resident CD8+ T cells (TRM) in tumors and their differential response to immunotherapy

  • Investigation of CD8+ TRM cell development in humanized mouse models

  • Harnessing tissue-resident CD8+ T cells for improved local tumor control

• Combination Therapy Optimization:

  • Evaluation of how checkpoint inhibitors, cytokine therapies, and targeted drugs modulate different CD8+ T cell subsets

  • Identification of optimal combination strategies based on CD8+ T cell phenotype changes

  • Development of sequential therapy approaches guided by CD8+ T cell functional status

• Single-Cell Multi-Omics Integration:

  • Correlation of CD8 protein expression with transcriptomic, epigenomic, and proteomic profiles at the single-cell level

  • Identification of molecular drivers of functionally distinct CD8+ T cell states

  • Development of computational models to predict CD8+ T cell functionality and therapeutic potential

• Humanized Model Refinement:

  • Advanced humanized mouse models with improved recapitulation of human CD8+ T cell development and function

  • Models enabling study of CD8+ T cell responses to cancer, infectious diseases, and autoimmunity

  • Platforms for testing novel immunotherapeutic approaches targeting specific CD8+ T cell subsets