Isolating and identifying cell populations are the first essential steps for manufacturing cells for cell-based tissue engineering approaches. Cell sorting is critical for the isolation and identification of cell populations and subpopulations with optimal cellular potency. Traditionally, endothelial cells and muscle satellite cells are isolated and sorted by distinct surface markers via label-based approaches, which involve tagging targets of interest with antibodies. The standard approach for isolating muscle satellite cells is to negatively select for non-myogenic cells (i.e., sort for CD31, CD45, Sca-1 negative cells) and positively select for certain markers (e.g., sort for α7-integrin positive cells) (Motohashi et al., 2014; Sincennes et al., 2017). Likewise, to isolate endothelial cells, immune and epithelial cells are depleted (i.e., remove CD45 and EpCAM cells), and endothelial cells are enriched (e.g., select for CD31 + cells) (Conchinha et al., 2021).

These label-based approaches are also commonly leveraged to identify subpopulations of cells with distinct functions. For example, single-cell RNA-seq of human satellite cells has identified subpopulations of cells, including CAV1⁺ cells, that are morphologically distinct and demonstrated enhanced cell engraftment upon transplantation (Barruet et al., 2020). Additionally, slow-dividing satellite cells isolated from mouse extensor digitorum longus muscle (identified by dilution of the membrane dye PKH26) demonstrated long-term self-renewal and enhanced contribution to muscle regeneration in vivo (Ono et al., 2012). Differences in the performance of subpopulations of endothelial cells have also been identified. In particular, endothelial cells with high CD34 expression have shown higher levels of IL-33 and Angiopoietin 2 production, which regulates their ability to induce Treg proliferation (Arakelian et al., 2023). These differences in subpopulation performance also extend to endothelial cell interactions with synthetic tissue-engineered vascular grafts, where cells with low FLRT2 expression have been shown to have a greater ability to adhere to the synthetic material (Wolfe et al., 2024).

However, these label-based approaches are limited by their cost and the persistence of sorting surface antibodies that can interfere with subsequent cell function, analysis, or testing. Label-free approaches, while less common, alleviate these limitations since they do not require antibody use. For example, label-free-inertial separation in microfluidic devices is increasingly utilized to isolate cell populations and have enriched for myogenic cells from a mixed population with larger fibroblast progenitors (Syverud et al., 2018). Unfortunately, label-free approaches for muscle and endothelial cells are limited and current approaches are low throughput; further development is needed before they are a practical and cost-effective alternative.

Obtaining the desired cell composition is often not sufficient to guarantee the efficacy of regenerative medicine and tissue engineering therapies. Measuring cell potency during manufacturing processes is critical for ensuring clinical success of the therapy. Moreover, the method of determining cell potency depends on the cell type being analyzed. Endothelial cell and endothelial progenitor cell potency is often characterized by the cells’ ability to form new blood vessel networks, whether it be de novo vessel formation (vasculogenesis) or vessel formation from pre-existing vessels (angiogenesis). Traditionally, the potency of these cells has been measured via intracellular markers, such as the expression of nitric oxide synthase (eNOS) and pro-angiogenic markers (VEGF, HGF, IGF-1) (Bouloumié et al., 1999; Sekiguchi et al., 2009). Alternatively, endothelial cell potency can be functionally measured by their in vitro capacity to form 3D vasculature structures of distinct architecture in physiologically relevant microenvironments. Measured geometric metrics of the formed vasculature, such as mean vessel length, number of junctions, and number of endpoints (van der Schaft et al., 2004; Zudaire et al., 2011) indicate a more actively regenerating phenotype.

In the case of satellite cells and muscle progenitor cells (i.e., myoblasts) that fuse into multinucleated myofibers (precursors of muscle fibers), a higher fusion index, number of nuclei per myofiber, presence of myosin heavy chain, and increased expression of CD56 cellular markers indicate high differentiation potency (Joulia et al., 2003; Shefer et al., 2006; Thurner et al., 2018). Moreover, muscle satellite cell potency is often measured by the cells’ in vivo engraftment potency in muscle injury models. However, the regular use of in vivo potency assays may not be practical. In the future, a shift to in vitro 3D physiologically relevant myogenic potency assays may be necessary.

Bioreactors control environmental conditions and allow for both dynamic cell culture and large-scale expansion of cells. These systems can control a variety of factors, including flow, nutrient supply, and loading of engineered cells and/or tissues. Shear stress, for example, has been shown to enhance the ability of iPSCs to mature into endothelial cells of an arterial-like phenotype (Sivarapatna et al., 2015). A more recent study has evaluated how different shear rates can influence the arterial markers NOTCH1 and EphrinB2 of human pluripotent stem cell-derived endothelial cells (Masumura et al., 2009).

Unfortunately, large-scale expansion of cells in simple flow bioreactors can be limited due to space. Thus, the use of hollow fibers and microcarriers in perfusion or stirred tank bioreactors have become increasingly utilized, as they increase culture surface area (Stephenson and Grayson, 2018; García-Fernández et al., 2020). In particular, the combination of 3D porous gelatin microcarriers and spinner flasks or stirred tank bioreactors has been shown to greatly improve long-term culture and large-scale expansion of muscle satellite cells and myoblasts (Liu et al., 2022). For example, bovine satellite cells demonstrated the ability to expand on CytoDEX microcarriers in a bench-top stir tank bioreactor over 38 days while maintaining their satellite cell phenotype via expression of Pax7 (Tzimorotas et al., 2023). However, future work will be necessary to overcome current limitations of bioreactors, which include contaminations due to complex platform design, difficulty monitoring and/or harvesting manufactured cells, complications with maintaining specific shear stresses, and overall cost. Each bioreactor design is susceptible to varying limitations based on the platform.

Distinct combinations of chemical factors and proteins have been shown to be critical to the large-scale expansion of regenerative muscle and endothelial cells while maintaining cellular potency in vitro and in vivo. For example, the growth factors EGF, bFGF, and HGF are critical for myoblasts’ proliferation, morphology, and fusion potential compared to commercially available media (SKGM-2) only containing hEGF (Jarocha et al., 2014). Moreover, vitamins and minerals, such as L-Ascorbic acid, also increase muscle stem cell proliferation while maintaining the cells’ ability to differentiate (Zhu et al., 2022). For umbilical cord blood-derived endothelial colony-forming cells, human platelet lysates have been shown to increase the viability, reduce the apoptosis, and increase the proliferation of the cells on a variety of different substrates (Denecke et al., 2015).

Improvements in the in vitro expansion of muscle stem cells with defined chemical cues have also been shown to enhance the cells’ engraftment in vivo. T-cell derived inflammatory cytokines, including IL-1α, IL-13, TNF-α, and IFN-γ, were shown to potently induce long-term expansion of muscle satellite cells in vitro over 20 passages. These cytokines also contribute to muscle regeneration in vivo, by improving continuous repair of muscle following multiple rounds of muscle injury (Fu et al., 2015). The combination of biochemical and biophysical cues, including a small-molecule inhibitor of p38α/p38β mitogen-activated protein kinase, and soft polyethylene glycol hydrogels, allowed for the expansion of functional muscle stem cells from aged mice. These functional muscle stem cells can be used to regenerate damaged muscle in an aged mouse population (Cosgrove et al., 2014). Overall, these chemical factors and proteins offer a promising method for maintaining cellular potency. However, their use can be limited due to the high cost of these materials and recombinant proteins, especially as depleted factors and proteins need replenished in culture.

Many gene editing approaches can be used for cell-based therapies to enhance cell function and potency, including zinc-finger proteins, transcription activator-like effector nucleases, and CRISPR-Cas9 (Ashmore-Harris and Fruhwirth, 2020). Particularly, gene editing approaches have been shown to improve cell function for regenerative medicine applications. For example, retroviral vectors have been used to induce insulin-like growth factor-I gene expression in myoblast cells to improve the contractile response of tissue constructs that the cells form (Sato et al., 2011). Furthermore, CRISPR-Cas9 gene editing is becoming a promising method for enhancing cellular potency. For example, CRISPR can confer certain advantages to cultured endothelial cells, such as resistance to TNF-α cytotoxicity via ablation of NLRX1 (Cai et al., 2019) and enhanced junctional integrity of formed blood vessels via ablation of the cytoplasmic domain of PECAM-1 (Liao et al., 2018). CRISPR/Cas9 has also been utilized to ablate class I major histocompatibility complex molecules, which allows endothelial cells to avoid activation of allogenic natural killer cells (Merola et al., 2019). The advantages of CRISPR-Cas9 have also extended to enhancing the potency of muscle progenitor cells. Specifically, dystrophin defects in iPSCs derived from patients with Duchenne muscular dystrophy were reversed with CRISPR-Cas9, resulting in normal myoblasts from the diseased patients (Young et al., 2016). Upregulation of IGF-1 expression with CRISPR-Cas9 in myoblasts also enhanced their differentiation and reduced DMSO-induced atrophy in vitro (Roberston et al., 2020). While CRISPR-Cas9 offers a promising method for cell manufacturing, it can be hindered by its high cost and low transfection efficiencies in primary cells. Furthermore, gene-editing technologies broadly may have off-target effects characterized by unintended edits outside of the target area.

The identity of the biomaterial substrate that regenerative cells are cultured on is a key determinant of their cellular potency during long-term expansion. These substrates, which include both synthetic and natural biomaterials, have been shown to be advantageous over traditional tissue culture polystyrene. Endothelial cells derived from pluripotent stem cells demonstrated greater expression of genes related to vessel development, ECM, and glycolysis when cultured in 3D thermoreversible PNIPAAM-Peg hydrogels compared to cultures on 2D Matrigel-coated plates (Lin et al., 2018). Natural polymers have also been utilized when manufacturing human pluripotent stem cell-derived endothelial cells in 3D alginate hydrogel tubes, which demonstrated higher expression of endothelial cell-related genes and rates of glycolysis (Lin et al., 2019). More recently, food-grade microcarriers made of collagen and eggshell membrane were shown to expand muscle stem cells and induce activated, proliferating muscle stem cells with altered cell adhesion patterns compared to stem cells expanded on conventional CytoDEX microcarriers (Andreassen et al., 2022). While natural materials have shown beneficial results for endothelial and muscle cells, reproducibility of natural substrates can be difficult due to the batch-to-batch variability. Monitoring of substrate variability when utilizing these types of substrates for cell manufacturing is necessary to ensure expected outcomes.

In addition to the identity of the cell substrate, specific cell culture surface modifications have been shown to improve cell morphology and proliferation while maintaining potency. Endothelial cells cultured on a matrix composed of fibrin, fibronectin, gelatin, and VEGF maintained greater proliferation potential and lower thrombogenic characteristics than endothelial cells cultured on gelatin after several passages (Prasad Chennazhy and Krishnan, 2005). Likewise, the expansion of mouse skeletal muscle progenitor cells on Matrigel-coated dishes resulted in higher proliferation and multinucleated myotubes compared to collagen-coated dishes (Shahini et al., 2018).

The mechanical properties of substrates can greatly affect cell growth and differentiation during cell expansion. The design of biomaterial mechanical properties can be fine-tuned to improve cell potency and culture. In particular, substrate stiffness has been extensively explored as a key parameter for cell expansion. For example, endothelial cells derived from various sources (umbilical vein, aorta, saphenous vein, and dermal microvasculature) demonstrated heterogeneous responses to hydrogel stiffness in terms of cell attachment, spreading, elongation, and proliferation (Wood et al., 2011). This is further illustrated for muscle progenitor cells, where soft hydrogels (12 kPa) improved cell potency, myoblast self-renewal in vitro, and muscle regeneration in vivo compared to culture on hard TCPS (10⁶ kPa) (Gilbert et al., 2010).

Furthermore, the viscoelasticity or elasticity of the material is critical to cell function and expansion. While not yet evaluated in the context of cell manufacturing, endothelial cells have been shown to be responsive to material viscoelasticity and plasticity in terms of their morphogenesis and proliferation (Shayan et al., 2023; Wei et al., 2023). Similar results have been observed for muscle progenitor cells. Specifically, an elastic chitosan/beta-glycerophosphate/collagen hydrogel mimicking the elastic modulus of muscle was used to expand myoblasts with greater proliferation capability, cell viability, colony-forming frequency, and potential for myogenic differentiation compared to myoblasts cultured on TCPS (Ding et al., 2015). The viscoelasticity and stress relaxation of the gel substrate have also been shown to greatly affect the proliferation and spreading of myoblasts. Namely, the stress-relaxing substrates resulted in greater spreading and proliferation of myoblasts compared to purely elastic substrates (Bauer et al., 2017). A significant hurdle when altering substrate mechanical properties is the ability to independently tune different mechanical properties of the materials, such as stiffness from viscoelasticity, which may be difficult based on the cross-linking chemistries of the material. This may inhibit the ability to match the native mechanical properties of certain in vivo tissues.

Across these diverse manufacturing methods, there are several existing limitations in manufacturing therapeutically potent cells for clinically relevant regenerative medicine therapies. For example, it remains a critical challenge to accurately recapitulate the complex chemical and physical microenvironment of native tissues during cell manufacturing protocols, which are likely required to maintain or improve cellular potency during in vitro expansion. Furthermore, there are significant hurdles in scaling the exponential expansion of these cell manufacturing approaches to meet the cell number and density needs of clinically sized, large-scale tissue-engineered constructs. For engineering tissues of high cellular density, such as skeletal muscle tissue, the manufacturing costs associated with producing large quantities cells (on the order of billions of cells) may make these engineered constructs prohibitively expensive. Furthermore, there is also significant variability in cell function across these diverse methods, further warranting improved standards and metrics for evaluating the function, potency, and in vivo integration of the cells and their resulting engineered constructs.

Living tissues are composed of a multitude of different cell types. Even within the same cell population of an organ, research has shown the existence of different clusters of differentiation or specialization (Rodor et al., 2022). To engineer and regenerate tissues that match the form and function of our native tissues, there is a need for improved approaches to characterize the properties of these cell subgroups to reproduce spatial tissue heterogeneity. To measure this heterogeneity for cell manufacturing and tissue engineering, emerging omics technologies, including single-cell RNA sequencing (scRNA-seq), single-cell spatial transcriptomics, and single-cell mass cytometry, can be leveraged. These approaches provide single-cell level resolution of individual cells’ gene expression and protein production, which can be used to infer information about their identity. Ultimately, omics technologies may broadly be useful in evaluating whether manufactured cells maintain their intrinsic cell variation both during cell manufacturing processes and after forming 3D tissues relative to their native source tissues and organs.

Single-cell RNAseq (scRNA-Seq) is a critical technology in next-generation sequencing that analyzes individual cell transcriptomes. The technique, first developed in 2009 (Tang et al., 2009), was an expansion of earlier techniques, namely, bulk-RNA sequencing, that allowed for the measurement of all actively synthesized proteins within a population. These approaches have been applied to endothelial cells and muscle stem cells in vivo and in vitro. For example, scRNA-seq has been used to measure the heterogeneity of organ-specific endothelial cell populations, which uncovered 13 transcriptomically distinct endothelial cell subpopulations independent of tissue origin (Paik et al., 2020). In addition to identifying different clusters of endothelial cells, scRNA-seq has identified 2 clusters of cultured corneal endothelial cells that expressed increased expression of the functional markers ALCAM and CDH2, identifying these subpopulations as cells with high therapeutic potential (Català et al., 2023).

In the context of myogenic cells, scRNA-seq has identified 17 different genetic clusters in myoblasts extracted from adult muscle tissue, all of which had differentially expressed surface markers and intracellular proteins. This analysis identified heterogeneity in the cells regarding muscular cell differentiation and ultimate cell fate, with specialized subpopulations that expressed unique signatures in terms of senescence, satellite cell quiescence, anti-inflammatory activity, and oxidative stress phenotypes. Of note, these differences were not associated with sex or age in mice and human populations (Barruet et al., 2020).

In the field of vascular tissue engineering, scRNA-seq has also been adopted to characterize heterogeneities in engineered vasculature in vitro and in vivo. Identification of the heterogeneous cellular composition of the tissues can provide insights into tissue health and whether the tissues replicate key functions observed in vivo. For example, in engineered microvasculature, sc-RNAseq identified heterogeneities in endothelial cells cultured in 3D engineered microvessels with either straight or spiral geometry under different flow regimens. This analysis revealed that flow in spiral vessels induced a unique subpopulation of endothelial cells not found in straight vessels, which modified gene expression related to angiogenesis, vascular growth, and inflammatory stress responses (Mandrycky et al., 2020). scRNA-seq was also utilized to validate a personalized tissue-engineered vein (P-TEV) derived from decellularized allogenic vena cava grafts that were reconditioned with autologous peripheral blood vessels in a pig model. The analysis revealed that post-implantation, the regenerated vena cava from the P-TEV exhibited single-cell gene expression profiles similar to native vena cava, highlighting the success of the approach in recapitulating native tissue heterogeneity (Österberg et al., 2023).

In the context of skeletal muscle tissue engineering, sc-RNAseq has validated the heterogeneity of satellite cells and myoblasts within engineered muscular tissue. Recently, scRNA-seq was utilized to identify both quiescent and activated satellite cell subpopulations within engineered 3D human myofibers (Wang et al., 2022). In a similar engineered muscle from human induced pluripotent stem cells, scRNA-seq analysis revealed cell subpopulations modeling muscle, mesenchyme, and neural lineage, demonstrating successful emulation of important neural muscle developmental stages in 2D and 3D microenvironments (Shahriyari et al., 2022).

Where scRNA-seq provides single-cell level analysis of protein expression, spatial transcriptomics indicates the distribution of one or multiple genes. These genes are labeled to determine the relative location of gene expression in relation to other cell types. The trade-off and limitation with this spatial information compared to scRNA-seq is that fewer genes can be analyzed at a time on a cell-to-cell basis (Ståhl et al., 2016). These analyses have thus far been applied to native or graft vasculature and muscle tissue in vivo in preclinical models. For example, spatial transcriptomics was used to identify the spatial architecture of activated cells in vein grafts following distension during harvesting, thus highlighting specific regions and subpopulations of cells that respond to distension (Michaud et al., 2024). Furthermore, spatial transcriptomics was used to measure diversity in endothelial cells from different organs in diabetic patients as compared to healthy individuals (Wang et al., 2024). Likewise, the same technology was used to identify the disease markers in histological samples for Duchenne Muscular Dystrophy and Muscular Sarcoidosis (Heezen et al., 2023; Larouche et al., 2023; Lequain et al., 2023). There is significant potential for using these approaches to characterize engineered tissues, measure cellular dispersion within biomaterials, and ultimately utilize this information for product quality control. By better characterizing spatial cellular identity and heterogeneity, it is possible to obtain insights into how cell populations are seeded throughout biomaterials or injury sites.

Lastly, mass cytometry is a combination of two previously used techniques: flow cytometry and mass spectroscopy. Cells are fixed and labeled using antibodies conjugated to heavy metal isotopes, which are then run through the traditional mass spectroscopy process to identify them. This approach benefits from the high resolution, multiplexed, high throughput capabilities of mass spectroscopy without the shortfalls of traditional fluorescence flow cytometry, such as signal decay and spectral overlap. However, it does have challenges, including sample disintegration and low sensitivity (Spitzer and Nolan, 2016). Through Imaging Mass Cytometry (IMC), a form of mass cytometry that adds a high-fidelity, image scan of the sample, it is possible to obtain single-cell spatial transcriptomics resolution with a marker count like scRNA-seq. These approaches have thus found utility for identifying cell diversity for fundamental studies in regeneration and cancer. This includes identification of cells involved in pancreatic ductal adenocarcinoma, where endothelial cells were found to be closely associated with stromal cells and distantly separated from tumor and ductal cells (Sussman et al., 2024). In the context of muscle cells, these approaches can reconstruct in vivo cell heterogeneity data of the myeloid lineage gastrocnemius (GA) and tibialis anterior (TA) muscles (Porpiglia et al., 2017), as well as evaluate differentiation and autophagy of in vitro cultured myoblast cells (Brown et al., 2021). However, these methods are limited by their cost, throughput, sensitivity, and resolution. As mass cytometry gains more widespread adoption and becomes more cost-effective, these approaches will also become adopted for characterizing engineered tissues.

Insights from the aforementioned omics technologies can pave the way for future approaches to utilize cell heterogeneity to engineer tissues that model the form and function of our native tissues. By leveraging innovative biomanufacturing techniques, researchers can manipulate cell diversity to achieve three general outcomes: 1) selectively choose specific cellular populations that are associated with particular tissue-forming capacities and/or positive patient outcomes (i.e., removing cells associated with fibrosis and chronic inflammation); 2) recapitulate native tissue structure by tailoring the proportions of specific cell subpopulations to reconstruct the native proportions or to a more favorable ratio for regeneration; 3) spatially reconstruct cell positioning with the advent of additive manufacturing techniques. These outcomes can be achieved via specific approaches, such as cell sorting, genetic engineering, and 3D bioprinting, which can manipulate cell variations to further improve cell potency and cell spatial localization (Figure 2). Engineering spatially organized and controlled tissues with these approaches is critical, as disorganized or varied cell populations are associated with certain disease states (Wu et al., 2022).

A proper understanding of cell variability and subpopulations can be leveraged to enrich specific cell groups that exhibit specific functions and/or tissue-forming capacity (Figure 2). For example, cell sorting of unique endothelial cell subpopulations identified by sc-RNAseq (Paik et al., 2020; Mandrycky et al., 2020) may be used to enrich for cells that self-assemble in blood vessels of distinct geometries (diameter, branching point, length), permeability, and antigen-presentation capacity. In the context of muscle stem cells, cell sorting may select cells identified from scRNA-seq (Barruet et al., 2020; Lovrić et al., 2022) that form muscle fibers of distinct shape, type, and contractile function. These approaches would overall provide tissue engineers greater control over tissues formed by cellular self-assembly at injury sites or in biomaterials. The expression of integrins (Kwee et al., 2021) and other cell adhesion proteins, such as cell cadherins, may also be targets for sorting out these unique subpopulations due to their critical role in tissue self-assembly and extracellular matrix remodeling. This would overall improve upon existing approaches to engineer self-assembled tissues in biomaterials that often yield tissues with a disorganized and random distribution of tissue structures.

With improved understanding of transcriptomics and molecular mechanisms underlying diverse cell groups, genetic engineering may be used for the targeting of specific gene(s) to manipulate cell diversity and variation (Figure 2). Specifically, cells can be genetically modified to alter the expression of key surface markers or genes that are representative of distinct cellular subpopulations with a particular function or tissue-forming capacity. Building off previous work, for example, satellite cells may be genetically modified to upregulate CAV1 to match the phenotype of CAV1+ satellite cell subpopulations that demonstrate enhanced engraftment and muscle formation in vivo (Barruet et al., 2020). Similarly, endothelial cells may be genetically modified to upregulate CD34 to enhance paracrine signaling function, due to identified cell subpopulations of high CD34 expression have increased IL-33 and Angiopoietin 2 production (Arakelian et al., 2023). Modulation of integrin expression, which has been utilized to identify cells in biomaterials of distinct potency, may also be a target for genetic manipulation to regulate cell potency in biomaterial scaffolds (Kwee et al., 2021). These genetic engineering approaches may provide a means to generate and manufacture large quantities of cells of a distinct subpopulation when the subpopulation of cells is limited in number and cannot be expanded in vitro.

The emergence of various 3D printing technologies offers a variety of biomanufacturing approaches to manipulate and form spatially heterogeneous tissues. 3D printing has been utilized extensively to precisely engineer the architecture and placement of cells and biomaterials for skeletal muscle (Choi et al., 2016) and vascular tissue engineering (Kolesky et al., 2016). In these existing approaches, different materials of varying composition, fiber alignment, and mechanical properties have been spatially organized with 3D printing (Choi et al., 2016). Furthermore, 3D printing has allowed for complex, multiscale vessel networks and positioning of different cell types in appropriate locations (Kolesky et al., 2014; 2016). Approaches have also been developed that allow 3D printing of distinct growth factors throughout engineered scaffolds, particularly to spatially localize distinct regions of blood vessel and bone formation (Freeman et al., 2020).

Moving forward, the 3D bioprinting of subpopulations of cells with distinct tissue-forming capacity can be leveraged to precisely seed cells throughout different locations of a biomaterial scaffold to form heterogeneous self-assembled tissues (Figure 2). For example, endothelial cell subpopulations with unique vessel-forming capacity may be spatially distributed throughout biomaterials to form self-assembled vasculature with spatial hierarchy of vessel geometries. This may lead to distinct regions where arteries/veins, arterioles/venules, and capillaries are formed by cellular self-assembly. Furthermore, spatially distribution of muscle progenitor cells within biomaterials may lead to self-assembled muscle fibers of defined distribution in muscle fiber type and size. This will be critical for engineering muscles that have specific and controlled contractile function, as muscle structural heterogeneity is critical for muscles to strain and contract in specific orientations (Azizi and Deslauriers, 2014).

A critical future direction in leveraging and manipulating these cell heterogeneities will be the creation of standards and metrics for measuring tissue and organ level heterogeneity and function. The standard metric for evaluating the heterogeneity of engineered tissues and cultured cells is to compare scRNA-seq analysis of the cells to scRNA-seq analysis of in vivo tissues and organs as a semi-qualitative metric of matching native tissue diversity. Comparison of engineered tissue and native spatial transcriptomics are also utilized as a metric of structural tissue heterogeneity, but this is limited by the 2D nature of these analyses. There is a critical need for improved approaches to measure cellular and tissue-level heterogeneity in 3D tissue structures in a robust manner. Furthermore, tissue and organ specific standards to evaluate the long-term function and integration of the engineered constructs are critical to demonstrate that the tissues also match the physiological diversity of the tissues. This may include standards to evaluate the ability of muscle to contract in different orientations or blood vessels to anastomosis with the host vasculature and deliver nutrients with similar efficacy as their native counterparts. Further development in these areas in conjunction with the enhanced cell manufacturing approaches described in this review are necessary for the clinical translation of cell-based tissue engineering.