The authors acknowledge&#160;the National Cancer Institute of the National Institutes of Health Pathway to Independence Award (K99CA201603).

The neonatal rat cardiomyocytes used in this protocol were isolated from 2-day-old Sprague-Dawley rats following a well-established procedure56 approved by the Institutional Animal Care and Use Committee at the Brigham and Women&#39;s Hospital.
1. Instrumentation of the Bioprinter
<ol>
	<li>Insert a smaller blunt needle (e.g., 27G, 1 inch) as the core into the center of a larger blunt needle (e.g., 18G, &#189; inch) as the sheath to construct the dual-layer, concentric microfluidic printhead; make sure that the core needle is protruding slightly (~1 mm) longer than the outer shell (Figure 1A). The alignment is usually adjusted manually, but if necessary spacers of proper sizes can be temporally sandwiched in between the inner/outer needles at both the tip and the barrel sides to assist concentric alignment. Seal the junction of the barrels with epoxy glue and remove the alignment spacers from the tip side when applicable.</li>
	<li>Insert another needle (23G) in the barrel of the central needle in the reverse direction.&#160; Then generate a hole on the side of the barrel of the outer needle and insert a metal connector of matching size into the hole, followed by sealing with epoxy glue.</li>
	<li>Connect the inlets of the printhead to a dual-channel syringe pump for injection of the bioink and the crosslinking solution, individually, through two PVC tubes. Mount the extruder onto the head of a bioprinter using a plastic holder made of poly(methyl methacrylate) (PMMA). 
	NOTE: Bioprinter selection depends on availability. In our case, we have successfully tested this setup on several commercially available bioprinters. However, any bioprinter that features an x-y-z motorized stage should, in principle, enable integration of this microfluidic printhead.</li>
</ol>
2. Bioprinting the Microfibrous Vascular Bed
<ol>
	<li>Make the bioink using a mixture of alginate (4 w/v%, low viscosity), gelatin methacryloyl (GelMA, 1-2 w/v%)57,58, and photoinitiator Irgacure 2959 (0.2 - 0.5 wt.%) dissolved in 25 mM 2-[4-(2-hydroxyethyl) piperazin-1-yl] ethane sulfonic acid (HEPES buffer, pH 7.4) containing 10 vol.% fetal bovine serum (FBS).</li>
	<li>Make a solution of 0.3-M CaCl2 in HEPES buffer containing 10 vol.% FBS as the crosslinking carrier fluid.</li>
	<li>Immediately before bioprinting, dissociate human umbilical vein endothelial cells (HUVECs) from the flasks using treatment by 0.05 w/v% trypsin for 5 - 10 min, and resuspend the cells in the bioink at a concentration of 5 - 10 &#215; 106 cells/mL. Pipette the suspension slowly 5 to 10 times to ensure homogenous distribution.</li>
	<li>Start the injection of the bioink/crosslinking fluid using a dual-channel syringe pump at the same flow rates of 5 &#181;L/mL. The flows can be allowed to continuously run for up to 1 min until they stabilize. Subsequently, initiate the movement of the printhead by controlling the bioprinter at a deposition speed of approximately 4 mm/s (Figure 1B). These speeds may need fine tuning with each new setup to ensure optimal bioprinting. The bioprinting process is usually conducted at room temperature (21 - 25 &#176;C) but this temperature may be altered. The bioprinting process should allow for fast ionic gelation of the alginate component and deposition of a microfibrous scaffold (Figure 1B).</li>
	<li>After the scaffold is bioprinted, achieve chemical gelation by further photocrosslinking the GelMA component, at approximately 5 - 10 mW/cm2 of UV light (360 - 480 nm) for 20 - 30 s (Figure 1C).</li>
	<li>Following the bioprinting and crosslinking, gently rinse the scaffold with phosphate-buffered saline (PBS) to remove the excess CaCl2. Culture the HUVECs-laden microfibrous scaffold in endothelial cell growth medium (EGM) in an incubator at 37 &#176;C and 5 vol.% CO2 for up to 16 days with medium changed at least every 2 days. Monitor the morphologies of the HUVECs under a microscope during the culture period.</li>
</ol>
3. Constructing the Vascularized Tissues
<ol>
	<li>Once the HUVECs have migrated to the peripheries of the microfibers in the scaffold to form the lumen-like structures (Figure 1D), retrieve the scaffold and gently place it on the surface of a hydrophobic surface (e.g., a slab of polymethylsiloxane [PDMS]). Use a piece of sterile filter paper to carefully remove all the medium from the interstitial space of the scaffold with capillary force.</li>
	<li>Immediately add a drop (approximately 20 - 40 &#181;L) of suspension of a secondary cell type (e.g., cardiomyocytes) in medium at a density of 1 - 10 &#215; 106 cells/mL on top of the scaffold, which should infiltrate the entire interstitial space of the scaffold (Figure 1E). Incubate such a configuration in an incubator (37 &#176;C, 5 vol.% CO2, 95% relative humidity) for 0.5 - 2 h to allow the cells to adhere onto the individual microfibers. Monitor the droplet size over the period to ensure that no noticeable evaporation is observed.</li>
	<li>Gently wash the scaffolds by shaking in a PBS bath to remove any non-adherent cells and culture the construct in relevant medium until the desired vascularized tissue is formed.</li>
</ol>

The authors declare that they have no competing financial interests.

Construction of the co-axial printhead represents a critical step towards successful microfluidic bioprinting to allow for simultaneous delivery of both the bioink from the core and the crosslinking agent from the sheath. While in this protocol an example printhead was created using a 27G needle as the core and an 18G needle as the shell, it may be readily extended to a variety of combinations using different sizes of needles. However, the alteration in the needle sizes, which results in the change in the amount of flow delivered in each phase, will require further optimization of the flow rates of both the bioink and the crosslinking agent (individually adjustable using two syringe pumps instead of a dual-channel one), and potentially also the deposition speed incurred by the bioprinter.
The combination of the parameters (needle sizes, flow rates, and deposition speed) in the current protocol led to the bioprinted microfibers with a diameter of approximately 120 &#181;m immediately after deposition, which would swell to roughly 150 &#181;m after equilibration in medium55. Such a size also roughly equals to the layer thickness of the bioprinted constructs as there was no space between the layers of the microfibers. The diameter of the bioprinted microfibers is a function of all three parameters54,63; the size of the core needle of the printhead and the flow rate of the bioink are positively correlated with the diameter of the microfibers, whereas the size of the sheath needle, the flow rate of the crosslinking agent, and the deposition speed are negatively correlated with the diameter of the microfibers. The control over the movement of the printhead and/or the motorized stage would allow for deposition of microfibrous scaffolds of arbitrary structures54,55.
Furthermore, the formulation of the bioink may change the profile of the bioprinting as well. For example, the amount of alginate and GelMA can be slightly modulated according to specific applications, and it is possible to blend additional materials into the bioink, such as polyethylene glycol-tetraacrylate (PEGTA) that increases the mechanics of the bioprinted microfibers40. The UV crosslinking also determines the mechanical properties of the center of the bioprinted microfibers, which can further affect the behavior of the embedded endothelial cells54. The parameters reported in this protocol was optimized for HUVECs. However, it is anticipated that, for each different type of endothelial cells the crosslinking parameters will need to be re-optimized to achieve lumen formation in the microfibers.
To seed a secondary cell type onto the bioprinted vascular bed, it is necessary to place the scaffold onto a piece of hydrophobic surface and ensure that most medium in the interstitial space of the scaffold is removed. This will allow immediate infiltration of the cell suspension into the microfibrous structure with the droplet free-standing and encapsulating the scaffold during the course of seeding, maximizing the number of cells attached onto the surface of the microfibers. Although a relatively high density of cardiomyocytes at 5 &#215; 106 cells/mL was used for constructing the myocardial tissue in the current protocol, such density can be arbitrarily tuned to match specific tissue types. It is also critical to maintain a humidified environment, which can be realized by filling sterile water or PBS in the vicinity of the scaffold (i.e., in the surrounding wells or the space surrounding the PDMS slab), ensuring that the small amount of medium for seeding does not evaporate over the period of seeding.
In summary, we have provided a detailed protocol of microfluidic bioprinting for convenient fabrication of vascularized tissues. In this strategy, a core-sheath co-axial printhead is used to enable simultaneous extrusion of a hybrid bioink from the core and crosslinking agent from the sheath. Upon co-extrusion, the bioink immediately undergoes physical crosslinking for its alginate component forming a layered microfibrous scaffold as programmed by the movement of the bioprinter, while the entire construct is further chemically photocrosslinked for the GelMA component to allow long-term stability. Endothelial cells encapsulated in the microfibers during the bioprinting process can proliferate and migrate to the peripheries assuming lumen-like structures, turning the scaffold into a vascular bed. By seeding a secondary cell type, a vascularized tissue construct can be subsequently generated. This microfluidic bioprinting strategy is unique, and can be conveniently extended to a variety of tissue types such as liver, skeletal muscle, and cancers besides the myocardium illustrated in the current protocol, by rational combination of desired cell types and specially designed patterns of the bioprinted microfibrous scaffolds. The vascularized tissue constructs produced with such a method may be used for in vivo tissue regeneration or for in vitro tissue modeling.
There are several limitations associated with the microfluidic bioprinting strategy described in this protocol. First, the diameter of the bioprinted microfibers is limited to a few hundred micrometers due to the diffusion barrier of the hydrogel matrix for the CaCl2 solution to efficiently crosslink the alginate component in the core. Overly low physical crosslinking density would make the multilayer structure unstable. Second, the physical crosslinking agent of CaCl2 solution may exert negative effects on certain endothelial cell types that are more fragile than HUVECs, such as the endothelial progenitor cells. The feasibility of using such a bioprinting method for a wider variety of endothelial cell types may require additional investigations. Third, while the endothelial cells can form lumen-like structures within the microfibers, the cores of these microfibers are not hollow to enable perfusion. Therefore, nutrients and oxygen are still provided mainly through the interstitial space in the bioprinted scaffolds. The adaptation of sacrificial materials as the photocrosslinkable component of the bioink64 may solve this issue in future versions of the technology. Alternatively, bioprinted hollow microfibrous structures42,43,65,66,67,68 may be used as the vascular bed to ensure direct perfusion of the vascularized tissue constructs. Last, bioprinting of clinical-sized tissues may still be challenging, which can likely be addressed by incorporating design of arrayed microfluidic printheads69 to achieve expanded-scale bioprinting at high throughput.

Tissue engineering targets to generate functional tissue substitutes that can be used to replace, restore, or augment those injured or diseased in the human body1,2,3,4, often through a combination of desired cell types, bioactive molecules5,6, and biomaterials7,8,9,10. More recently, tissue engineering technologies have also been increasingly adopted to generate in vitro tissue and organ models that mimic the important functions of their in vivo counterparts, for applications such as drug development, in replacement of the conventional over-simplified planar cell cultures11,12,13,14,15,16,17,18,19. In both situations, the ability to recapitulate the complex microarchitecture and hierarchical structure of the human tissues is critical in enabling functionality of the engineered tissues10, and in particular, ways to integrate a vascular network into the engineered tissues are of demand since vascularization presents one of the greatest challenges to the field20,21,22,23.
To date, a variety of approaches have been developed in this regard in an attempt to build blood vessel structures into engineered tissue constructs with various degrees of success8. For example, self-assembly of endothelial cells allows for generation of microvascular networks24; delivery of angiogenic growth factors induces sustained neovascularization25,26; use of vascular progenitor cells and pericytes facilitates endothelial cell growth and assembly24,27; designing scaffold properties enables precise modulation of vascularization28,29; and cell sheet technology allows for convenient manipulation of vascular layering30. Nevertheless, these strategies do not endow the capability of controlling the spatial patterning of the vasculature, often leading to random distribution of blood vessels within an engineered tissue construct and thus limited reproducibility. During the past few years bioprinting has emerged as a class of enabling technologies towards the solution of such a challenge, due to their unparalleled versatility of depositing complex tissue patterns at high fidelity and reproducibility in an automated or semi-automated manner31,32,33. Sacrificial bioprinting34,35,36,37,38, embedded bioprinting39,40,41, and hollow structure bioprinting/biofabrication42,43,44,45,46,47,48,49,50,51,52,53 have all demonstrated the feasibility of generating vascular or vascularized tissues.
Alternatively, a microfluidic bioprinting strategy to fabricate microfibrous scaffolds have been recently developed, where a hybrid bioink composed of alginate and gelatin methacryloyl (GelMA) was delivered through the core of a concentric printhead and a calcium chloride (CaCl2) solution was carried through the outer sheath flow of the printhead54,55. The co-extrusion of the two flows allowed for immediate physical crosslinking of the alginate component to enable microfiber formation, while subsequent photocrosslinking ensured permanent stabilization of the multi-layer microfibrous scaffold. Of note, endothelial cells encapsulated within the bioprinted microfibers were found to proliferate and migrate towards the peripheries of the microfibers assuming lumen-like structures that mimicked the vascular bed54,55. These bioprinted, endothelialized vascular beds could be subsequently populated with desired secondary cell types to further construct vascularized tissues55. This protocol thus provides a detailed procedure of such a microfluidic bioprinting strategy enabled by the concentric nozzle design, which ensures convenient fabrication of vascularized tissues for potential applications in both tissue engineering and organoid modeling.

<table><tbody><tr><td>Alginic acid sodium salt from brown algae</td><td>Sigma-Aldrich</td><td>A0682</td><td>BioReagent, plant cell culture tested, low viscosity, powder</td></tr><tr><td>Gelatin type A from porcine skin</td><td>Sigma-Aldrich</td><td>G2500</td><td>Gel strength 300</td></tr><tr><td>Irgacure 2959 (2-Hydroxy-4&#039;-(2-hydroxyethoxy)-2-methylpropiophenone)</td><td>Sigma-Aldrich</td><td>410896</td><td>98%</td></tr><tr><td>HEPES buffer</td><td>Sigma-Aldrich</td><td>H0887</td><td>1 M, pH 7.0 - 7.6, sterile-filtered, BioReagent, suitable for cell culture</td></tr><tr><td>Fetal bovine serum&amp;nbsp;</td><td>Thermo Fisher Scientific</td><td>10438026</td><td>Qualified, heat-inactivated, USDA-approved regions</td></tr><tr><td>Calcium chloride dihydrate</td><td>Sigma-Aldrich</td><td>C5080</td><td>BioXtra, &amp;ge;99.0%</td></tr><tr><td>Phosphate buffered saline</td><td>Thermo Fisher Scientific</td><td>10010023</td><td>pH 7.4</td></tr><tr><td>Human umbilical vein endothelial cells</td><td>Angio-Proteomie</td><td>cAP-0001</td><td>Human Umbilical Vein Endothelial Cells (HUVECs)</td></tr><tr><td>GFP-expressing human umbilical vein endothelial cells</td><td>Angio-Proteomie</td><td>cAP-0001GFP</td><td>GFP-Expressing Human Umbilical Vein Endothelial Cells (GFPHUVECs)</td></tr><tr><td>Endothelial cell growth medium</td><td>Lonza</td><td>CC-3162</td><td>EGM-2 BulletKit</td></tr><tr><td>Dulbecco&amp;rsquo;s Modified Eagle Medium&amp;nbsp;</td><td>Thermo Fisher Scientific</td><td>12430054</td><td>High glucose, HEPES</td></tr><tr><td>Sylgard 184 silicone elastomer kit</td><td>Ellsworth Adhesives</td><td>184 SIL ELAST KIT 0.5KG</td><td>Clear 0.5 kg Kit</td></tr><tr><td>UV curing lamp system</td><td>Excelitas Technologies</td><td>OmniCure S2000</td><td>Spot UV Light Curing System with Intelligent UV Sensor</td></tr></tbody></table>

microfluidic bioprinting for engineering vascularized tissues and organoids

Engineering vascularized tissue constructs and organoids has been historically challenging. Here we describe a novel method based on microfluidic bioprinting to generate a scaffold with multilayer interlacing hydrogel microfibers. To achieve smooth bioprinting, a core-sheath microfluidic printhead containing a composite bioink formulation extruded from the core flow and the crosslinking solution carried by the sheath flow, was designed and fitted onto the bioprinter. By blending gelatin methacryloyl (GelMA) with alginate, a polysaccharide that undergoes instantaneous ionic crosslinking in the presence of select divalent ions, followed by a secondary photocrosslinking of the GelMA component to achieve permanent stabilization, a microfibrous scaffold could be obtained using this bioprinting strategy. Importantly, the endothelial cells encapsulated inside the bioprinted microfibers can form the lumen-like structures resembling the vasculature over the course of culture for 16 days. The endothelialized microfibrous scaffold may be further used as a vascular bed to construct a vascularized tissue through subsequent seeding of the secondary cell type into the interstitial space of the microfibers. Microfluidic bioprinting provides a generalized strategy in convenient engineering of vascularized tissues at high fidelity.

The microfluidic bioprinting strategy allows for direct extrusion bioprinting of microfibrous scaffolds using low-viscosity bioinks54,55. As illustrated in Figure 2A, a scaffold with a size of 6 &#215; 6 &#215; 6 mm3 containing &#62;30 layers of microfibers could be bioprinted within 10 min. The immediate ionic crosslinking of the alginate component with CaCl2 allowed for excellent structural integrity during the bioprinting process while the subsequent physical photocrosslinking of the GelMA component ensured long-term stability of the bioprinted microfibrous scaffold, as indicated in top view and side view shown in Figures 2B and 2C. The microfibers achieved in this case, under the bioprinting conditions specified in the protocol, were approximately 100 - 150 &#181;m in diameter, which would slightly increase overtime with swelling.
The bioprinting process, including the microfluidic extrusion of the bioink, the ionic crosslinking, and the photocrosslinking, did not significantly affect the viability of the encapsulated HUVECs. The cells could maintain a relatively high viability of &#62;80% after completion of all these procedures (Figure 2D). As reported earlier54,55, the HUVECs could gradually proliferate and migrate in the microfibers from the initially random distribution at Day 0 (Figure 2E) to the peripheries of the microfibers to assume lumen-like structures at Day 16 post-bioprinting in culture (Figure 2F). Such a behavior observed for the HUVECs was likely due to the intrinsic interface-driven tendency of the endothelial cells as well as the higher availability of nutrients and oxygen surrounding the microfibers than in their interiors55,59.
The microfibrous scaffold can also function as a standalone platform for tissue engineering. Using myocardium tissue as an example, neonatal rat cardiomyocytes were seeded onto the interstitial space of a bioprinted scaffold at a density of 5 &#215; 106 cells/mL, and cultured in Dulbecco&#39;s Modified Eagle Medium (DMEM) supplemented with 10 vol.% FBS. The medium was changed every day in the first 2 - 3 days until the cardiomyocytes started beating, after which only &#189; medium was exchanged every 2 - 3 days55,60,61,62. The cells could maintain their spontaneous and synchronized beating for up to 9-28 days depending on the cell source and configuration of the scaffolds55. The mature cardiomyocytes on the scaffold also showed strong expression of functional cardiac biomarkers as illustrated in the confocal fluorescence images in Figure 3, including sarcomeric &#945;-actinin (Figure 3B) and connexin-43 (Figure 3C).
Combining the endothelial cells and the secondary cell type, a vascularized tissue could be further constructed. Again, using myocardium as an example, after the vascular bed has formed in a bioprinted microfibrous scaffold after roughly 16 days of culture, neonatal rat cardiomyocytes were subsequently seeded into the interstitial space of the scaffold. After culturing and maturation in a common medium composed of 1:1 volume ration of EGM:DMDM, an endothelialized myocardial tissue could be formed exhibiting spontaneous and synchronous beating55. Single-plane confocal fluorescence images in Figure 4 further revealed co-existence of both cell types, with the HUVECs mainly present in the boundaries of the microfibers (Figure 4B) and the cardiomyocytes surrounding the exteriors of the microfibers (Figure 4C).
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/55957/55957fig1.jpg" /> 
Figure 1: The Microfluidic Bioprinting Strategy for Generating Vascularized Tissue Constructs. 
(A)The design of the core-sheath coaxial printhead for co-extrusion of the composite bioink and the CaCl2. (B-E) Schematics showing the fabrication procedure of a vascularized tissue construct. This figure has been modified with permission from Ref.55. <a href="https://cloudflare-jove-com.bdigitaluss.remotexs.co/files/ftp_upload/55957/55957fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/55957/55957fig2.jpg" /> 
Figure 2: Bioprinting the Microfibrous Vascular Bed. 
(A) Photograph showing a bioprinted 30-layer microfibrous scaffold. (B, C) Top and side views of micrographs showing a bioprinted scaffold. (D) Viability of HUVECs laden in a bioprinted microfibrous scaffold. Green and red indicate live and dead cells, respectively. (E, F) Fluorescence micrographs showing the organization of green fuorescent protein (GFP)-HUVECs in the bioprinted microfibers at Day 0 and Day 16 post bioprinting, respectively. <a href="https://cloudflare-jove-com.bdigitaluss.remotexs.co/files/ftp_upload/55957/55957fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/55957/55957fig3.jpg" /> 
Figure 3: Subsequent Growth of Cardiomyocytes on the Bioprinted Microfibrous Scaffold. 
Fluorescence micrographs showing (A) nuclei, (B) sarcomeric &#945;-actinin, (C) connexin-43, and (D) superimposition. <a href="https://cloudflare-jove-com.bdigitaluss.remotexs.co/files/ftp_upload/55957/55957fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 4" class="xfigimg" src="/files/ftp_upload/55957/55957fig4.jpg" /> 
Figure 4: Construction of Endothelialized Myocardial Tissue. 
Fluorescence micrographs showing (A) nuclei, (B) GFP-HUVECs, (C) f-actin of both HUVECs and cardiomyocytes, and (D) superimposition. Inset in D shows a lower-magnification image of the endothelialized myocardial tissue. <a href="https://cloudflare-jove-com.bdigitaluss.remotexs.co/files/ftp_upload/55957/55957fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
Supplementary Dataset. 
A sample G-code file for bioprinting a 6 &#215; 6 mm2 square lattice with 220 &#181;m spacing between adjacent microfibers.

Watch this Scientific Journal Video about Microfluidic Bioprinting for Engineering Vascularized Tissues and Organoids at JoVE.com

Microfluidic Bioprinting for Engineering Vascularized Tissues and Organoids

We provide a generalized protocol based on a microfluidic bioprinting strategy for engineering a microfibrous vascular bed, where a secondary cell type could be further seeded into the interstitial space of this microfibrous structure to generate vascularized tissues and organoids.

Engineering vascularized tissue constructs and organoids has been historically challenging. Here we describe a novel method based on microfluidic ...

microfluidic-bioprinting-for-engineering-vascularized-tissues

Universidad San Sebastian

Research

JoVE Journal

Bioengineering

15.7K Views.  Harvard Medical School. We provide a generalized protocol based on a microfluidic bioprinting strategy for engineering a microfibrous vascular bed, where a secondary cell type could be further seeded into the interstitial space of this microfibrous structure to generate vascularized tissues and organoids.

Video: Microfluidic Bioprinting for Engineering Vascularized Tissues and Organoids

Viability of Bioprinted Cellular Constructs Using a Three Dispenser Cartesian Printer

Tissue engineering has centralized its focus on the construction of replacements for non-functional or damaged tissue. The utilization of three-dimensional bioprinting in tissue engineering has generated new methods for the printing of cells and matrix to fabricate biomimetic tissue constructs. The solid freeform fabrication (SFF) method developed for three-dimensional bioprinting uses an additive manufacturing approach by depositing droplets of cells and hydrogels in a layer-by-layer fashion. Bioprinting fabrication is dependent on the specific placement of biological materials into three-dimensional architectures, and the printed constructs should closely mimic the complex organization of cells and extracellular matrices in native tissue. This paper highlights the use of the Palmetto Printer, a Cartesian bioprinter, as well as the process of producing spatially organized, viable constructs while simultaneously allowing control of environmental factors. This methodology utilizes computer-aided design and computer-aided manufacturing to produce these specific and complex geometries. Finally, this approach allows for the reproducible production of fabricated constructs optimized by controllable printing parameters.

A Cartesian bioprinter was designed and fabricated to allow multi-material deposition in precise, reproducible geometries, while also allowing control of environmental factors. Utilizing the three-dimensional bioprinter, complex and viable constructs may be printed and easily reproduced.

Tissue engineering has centralized its focus on the construction of replacements for non-functional or damaged tissue. The utilization of ...

Bioprinting Cellularized Constructs Using a Tissue-specific Hydrogel Bioink

Bioprinting has emerged as a versatile biofabrication approach for creating tissue engineered organ constructs. These constructs have potential use as organ replacements for implantation in patients, and also, when created on a smaller size scale as model "organoids" that can be used in in vitro systems for drug and toxicology screening.
Despite development of a wide variety of bioprinting devices, application of bioprinting technology can be limited by the availability of materials that both expedite bioprinting procedures and support cell viability and function by providing tissue-specific cues. Here we describe a versatile hyaluronic acid (HA) and gelatin-based hydrogel system comprised of a multi-crosslinker, 2-stage crosslinking protocol, which can provide tissue specific biochemical signals and mimic the mechanical properties of in vivo tissues. 
Biochemical factors are provided by incorporating tissue-derived extracellular matrix materials, which include potent growth factors. Tissue mechanical properties are controlled combinations of PEG-based crosslinkers with varying molecular weights, geometries (linear or multi-arm), and functional groups to yield extrudable bioinks and final construct shear stiffness values over a wide range (100 Pa to 20 kPa). Using these parameters, hydrogel bioinks were used to bioprint primary liver spheroids in a liver-specific bioink to create in vitro liver constructs with high cell viability and measurable functional albumin and urea output. This methodology provides a general framework that can be adapted for future customization of hydrogels for biofabrication of a wide range of tissue construct types.

We describe a set of protocols that together provide a tissue-mimicking hydrogel bioink with which functional and viable 3-D tissue constructs can be bioprinted for use in in vitro screening applications.

Bioprinting has emerged as a versatile biofabrication approach for creating tissue engineered organ constructs. These constructs have potential use as ...

Micropatterning and Assembly of 3D Microvessels

In vitro platforms to study endothelial cells and vascular biology are largely limited to 2D endothelial cell culture, flow chambers with polymer or glass based substrates, and hydrogel-based tube formation assays. These assays, while informative, do not recapitulate lumen geometry, proper extracellular matrix, and multi-cellular proximity, which play key roles in modulating vascular function. This manuscript describes an injection molding method to generate engineered vessels with diameters on the order of 100 &#181;m. Microvessels are fabricated by seeding endothelial cells in a microfluidic channel embedded within a native type I collagen hydrogel. By incorporating parenchymal cells within the collagen matrix prior to channel formation, specific tissue microenvironments can be modeled and studied. Additional modulations of hydrodynamic properties and media composition allow for control of complex vascular function within the desired microenvironment. This platform allows for the study of perivascular cell recruitment, blood-endothelium interactions, flow response, and tissue-microvascular interactions. Engineered microvessels offer the ability to isolate the influence from individual components of a vascular niche and precisely control its chemical, mechanical, and biological properties to study vascular biology in both health and disease.

This manuscript presents an injection molding method to engineer microvessels that recapitulate physiological properties of endothelium. The microfluidic-based process creates patent 3D vascular networks with tailorable conditions, such as flow, cellular composition, geometry, and biochemical gradients. The fabrication process and examples of potential applications are described.

In vitro platforms to study endothelial cells and vascular biology are largely limited to 2D endothelial cell culture, flow chambers with polymer or glass ...

Image-guided, Laser-based Fabrication of Vascular-derived Microfluidic Networks

This detailed protocol outlines the implementation of image-guided, laser-based hydrogel degradation for the fabrication of vascular-derived microfluidic networks embedded in PEGDA hydrogels. Here, we describe the creation of virtual masks that allow for image-guided laser control; the photopolymerization of a micromolded PEGDA hydrogel, suitable for microfluidic network fabrication and pressure head-driven flow; the setup and use of a commercially available laser scanning confocal microscope paired with a femtosecond pulsed Ti:S laser to induce hydrogel degradation; and the imaging of fabricated microfluidic networks using fluorescent species and confocal microscopy. Much of the protocol is focused on the proper setup and implementation of the microscope software and microscope macro, as these are crucial steps in using a commercial microscope for microfluidic fabrication purposes that contain a number of intricacies. The image-guided component of this technique allows for the implementation of 3D image stacks or user-generated 3D models, thereby allowing for creative microfluidic design and for the fabrication of complex microfluidic systems of virtually any configuration. With an expected impact in tissue engineering, the methods outlined in this protocol could aid in the fabrication of advanced biomimetic microtissue constructs for organ- and human-on-a-chip devices. By mimicking the complex architecture, tortuosity, size, and density of in vivo vasculature, essential biological transport processes can be replicated in these constructs, leading to more accurate in vitro modeling of drug pharmacokinetics and disease.

This protocol outlines the implementation of image-guided, laser-based hydrogel degradation to fabricate vascular-derived, biomimetic microfluidic networks embedded in poly(ethylene glycol) diacrylate (PEGDA) hydrogels. These biomimetic microfluidic systems may be useful for tissue engineering applications, generation of in vitro disease models, and fabrication of advanced "on-a-chip" devices.

This detailed protocol outlines the implementation of image-guided, laser-based hydrogel degradation for the fabrication of vascular-derived microfluidic ...

Bioprinting of Cartilage and Skin Tissue Analogs Utilizing a Novel Passive Mixing Unit Technique for Bioink Precellularization

Bioprinting is a powerful technique for the rapid and reproducible fabrication of constructs for tissue engineering applications. In this study, both cartilage and skin analogs were fabricated after bioink pre-cellularization utilizing a novel passive mixing unit technique. This technique was developed with the aim to simplify the steps involved in the mixing of a cell suspension into a highly viscous bioink. The resolution of filaments deposited through bioprinting necessitates the assurance of uniformity in cell distribution prior to printing to avoid the deposition of regions without cells or retention of large cell clumps that can clog the needle. We demonstrate the ability to rapidly blend a cell suspension with a bioink prior to bioprinting of both cartilage and skin analogs. Both tissue analogs could be cultured for up to 4 weeks. Histological analysis demonstrated both cell viability and deposition of tissue specific extracellular matrix (ECM) markers such as glycosaminoglycans (GAGs) and collagen I respectively.

Cartilage and skin analogs were bioprinted using a nanocellulose-alginate based bioink. The bioinks were cellularized prior to printing via a single step passive mixing unit. The constructs were demonstrated to be uniformly cellularized, have high viability, and exhibit favorable markers of differentiation.

Bioprinting is a powerful technique for the rapid and reproducible fabrication of constructs for tissue engineering applications. In this study, both ...

Advancing 3D Bioprinting with &#954;-Carrageenan Sub-Microgel Medium

Embedded Bioprinting of Tissue-like Structures Using &#954;-Carrageenan Sub-Microgel Medium

Embedded three-dimensional (3D) bioprinting utilizing a granular hydrogel supporting bath has emerged as a critical technique for creating biomimetic scaffolds. However, engineering a suitable gel suspension medium that balances precise bioink deposition with cell viability and function presents multiple challenges, particularly in achieving the desired viscoelastic properties. Here, a novel &#954;-carrageenan gel supporting bath is fabricated through an easy-to-operate mechanical grinding process, producing homogeneous sub-microscale particles. These sub-microgels exhibit typical Bingham flow behavior with small yield stress and rapid shear-thinning properties, which facilitate the smooth deposition of bioinks. Moreover, the reversible gel-sol transition and self-healing capabilities of the &#954;-carrageenan microgel network ensure the structural integrity of printed constructs, enabling the creation of complex, multi-layered tissue structures with defined architectural features. Post-printing, the &#954;-carrageenan sub-microgels can be easily removed by a simple phosphate-buffered saline wash. Further bioprinting with cell-laden bioinks demonstrates that cells within the biomimetic constructs have a high viability of 92% and quickly extend pseudopodia, as well as maintain robust proliferation, indicating the potential of this bioprinting strategy for tissue and organ fabrication. In summary, this novel &#954;-carrageenan sub-microgel medium emerges as a promising avenue for embedded bioprinting of exceptional quality, bearing profound implications for the in vitro development of engineered tissues and organs.

Author Spotlight: Development of Homogeneous &#954;-Carrageenan Sub-Microgel Baths for High-Resolution 3D Bioprinting

This study introduces a novel &#954;-carrageenan sub-microgel suspension bath, displaying remarkable reversible jamming-unjamming transition properties. These attributes contribute to the construction of biomimetic tissues and organs in embedded 3D bioprinting. The successful printing of heart/esophageal-like tissues with high resolution and cell growth demonstrates high-quality bioprinting and tissue engineering applications.

Embedded three-dimensional (3D) bioprinting utilizing a granular hydrogel supporting bath has emerged as a critical technique for creating biomimetic ...

Engineering

Perfusable Vascular Network with a Tissue Model in a Microfluidic Device

A spheroid (a multicellular aggregate) is regarded as a good model of living tissues in the human body. Despite the significant advancement in the spheroid cultures, a perfusable vascular network in the spheroids remains a critical challenge for long-term culture required to maintain and develop their functions, such as protein expressions and morphogenesis. The protocol presents a novel method to integrate a perfusable vascular network within the spheroid in a microfluidic device. To induce a perfusable vascular network in the spheroid, angiogenic sprouts connected to microchannels were guided to the spheroid by utilizing angiogenic factors from human lung fibroblasts cultured in the spheroid. The angiogenic sprouts reached the spheroid, merged with the endothelial cells co-cultured in the spheroid, and formed a continuous vascular network. The vascular network could perfuse the interior of the spheroid without any leakage. The constructed vascular network may be further used as a route for supply of nutrients and removal of waste products, mimicking blood circulation in vivo. The method provides a new platform in spheroid culture toward better recapitulation of living tissues.

The protocol describes how to engineer a perfusable vascular network in a spheroid. The spheroid's surrounding microenvironment is devised to induce angiogenesis and connect the spheroid to the microchannels in a microfluidic device. The method allows the perfusion of the spheroid, which is a long-awaited technique in three-dimensional cultures.

A spheroid (a multicellular aggregate) is regarded as a good model of living tissues in the human body. Despite the significant advancement in the ...

Core/shell Printing Scaffolds For Tissue Engineering Of Tubular Structures

Three-dimensional (3D) printing of core/shell filaments allows direct fabrication of channel structures with a stable shell that is cross-linked at the interface with a liquid core. The latter is removed post-printing, leaving behind a hollow tube. Integrating an additive manufacturing technique (like the one described here with tailor-made [bio]inks, which structurally and biochemically mimic the native extracellular matrix [ECM]) is an important step towards advanced tissue engineering. However, precise fabrication of well-defined structures requires tailored fabrication strategies optimized for the material in use. Therefore, it is sensible to begin with a set-up that is customizable, simple-to-use, and compatible with a broad spectrum of materials and applications. This work presents an easy-to-manufacture core/shell nozzle with luer-compatibility to explore core/shell printing of woodpile structures, tested with a well-defined, alginate-based scaffold material formulation.

Presented here is a simple-to-use, core/shell, three-dimensional bioprinting set-up for one-step fabrication of hollow scaffolds, suitable for tissue engineering of vascular and other tubular structures.

Three-dimensional (3D) printing of core/shell filaments allows direct fabrication of channel structures with a stable shell that is cross-linked at the ...

Direct Bioprinting of 3D Multicellular Breast Spheroids onto Endothelial Networks

Bioprinting is emerging as a promising tool to fabricate 3D human cancer models that better recapitulate critical hallmarks of in vivo tissue architecture. In current layer-by-layer extrusion bioprinting, individual cells are extruded in a bioink together with complex spatial and temporal cues to promote hierarchical tissue self-assembly. However, this biofabrication technique relies on complex interactions among cells, bioinks and biochemical and biophysical cues. Thus, self-assembly may take days or even weeks, may require specific bioinks, and may not always occur when there is more than one cell type involved. We therefore developed a technique to directly bioprint pre-formed 3D breast epithelial spheroids in a variety of bioinks. Bioprinted pre-formed 3D breast epithelial spheroids sustained their viability and polarized architecture after printing. We additionally printed the 3D spheroids onto vascular endothelial cell networks to create a co-culture model. Thus, the novel bioprinting technique rapidly creates a more physiologically relevant 3D human breast model at lower cost and with higher flexibility than traditional bioprinting techniques. This versatile bioprinting technique can be extrapolated to create 3D models of other tissues in additional bioinks.

The goal of this protocol is to directly bioprint breast epithelial cells as multicellular spheroids onto pre-formed endothelial networks to rapidly create 3D breast-endothelial co-culture models which can be used for drug screening studies.

Bioprinting is emerging as a promising tool to fabricate 3D human cancer models that better recapitulate critical hallmarks of in vivo tissue ...

Fabrication of Engineered Vascular Flaps Using 3D Printing Technologies

Engineering implantable, functional, thick tissues requires designing a hierarchical vascular network. 3D bioprinting is a technology used to create tissues by adding layer upon layer of printable biomaterials, termed bioinks, and cells in an orderly and automatic manner, which allows for creating highly intricate structures that traditional tissue engineering techniques cannot achieve. Thus, 3D bioprinting is an appealing in vitro approach to mimic the native vasculature complex structure, ranging from millimetric vessels to microvascular networks. 
Advances in 3D bioprinting in granular hydrogels enabled the high-resolution extrusion of low-viscosity extracellular matrix-based bioinks. This work presents a combined 3D bioprinting and sacrificial mold-based 3D printing approach for fabricating engineered vascularized tissue flaps. 3D bioprinting of endothelial and support cells using recombinant collagen-methacrylate bioink within a gelatin support bath is utilized for the fabrication of a self-assembled capillary network. This printed microvasculature is assembled around a mesoscale vessel-like porous scaffold, fabricated using a sacrificial 3D printed mold, and is seeded with endothelial cells. 
This assembly induces the endothelium of the mesoscale vessel to anastomose with the surrounding capillary network, establishing a hierarchical vascular network within an engineered tissue flap. The engineered flap is then directly implanted by surgical anastomosis to a rat femoral artery using a cuff technique. The described methods can be expanded for the fabrication of various vascularized tissue flaps for use in reconstruction surgery and vascularization studies.

Engineered flaps require an incorporated functional vascular network. In this protocol, we present a method of fabricating a 3D printed tissue flap containing a hierarchical vascular network and its direct microsurgical anastomoses to rat femoral artery.

Engineering implantable, functional, thick tissues requires designing a hierarchical vascular network. 3D bioprinting is a technology used to create ...