Microfluidic oxygen control confers more than just convenience and speed over hypoxic chambers for biological experiments. Especially when implemented via diffusion through a membrane, microfluidic oxygen can provide simultaneous liquid and gas phase modulations at the microscale-level. This technique enables dynamic multi-parametric experiments critical for studying islet pathophysiology.
Simultaneous oxygenation and monitoring of glucose stimulus-secretion coupling factors in a single technique is critical for modeling pathophysiological states of islet hypoxia, especially in transplant environments. Standard hypoxic chamber techniques cannot modulate both stimulations at the same time nor provide real-time monitoring of glucose stimulus-secretion coupling factors. To address these difficulties, we applied a multilayered microfluidic technique to integrate both aqueous and gas phase modulations via a diffusion membrane. This creates a stimulation sandwich around the microscaled islets within the transparent polydimethylsiloxane (PDMS) device, enabling monitoring of the aforementioned coupling factors via fluorescence microscopy. Additionally, the gas input is controlled by a pair of microdispensers, providing quantitative, sub-minute modulations of oxygen between 0-21%. This intermittent hypoxia is applied to investigate a new phenomenon of islet preconditioning. Moreover, armed with multimodal microscopy, we were able to look at detailed calcium and KATP channel dynamics during these hypoxic events. We envision microfluidic hypoxia, especially this simultaneous dual phase technique, as a valuable tool in studying islets as well as many ex vivo tissues.
Dynamic hypoxia is important in biology, specifically for islet transplants
Dynamic hypoxia is an important physiological as well as pathophysiological parameter in many biological tissues. Change in oxygen, for example, is a potent developmental signal in angiogenesis. Moreover, spatial and temporal patterns in hypoxia modulate HIF1-alpha and play roles in diseases like pancreatic cancer. Hypoxia is also a confounding factor affecting islet transplant outcomes. Recently, temporally oscillations of hypoxia, or intermittent hypoxia (IH) have demonstrated benefits in "preconditioning" islets1. However, both static and transient hypoxia effects on islet physiology have yet to be well understood or studied, primarily due to the lack of appropriate tools to control islet's microenvironment.
Islets are well vascularized in vivo
Pancreatic islets are 50-400 μm spheroidal aggregates of endocrine cells, including beta-cells and alpha-cells that are responsible for glucose homeostasis. When islets are exposed to stimulatory glucose in the blood, uptake and glycolysis lead to ATP production, which opens up ATP-sensitive potassium (KATP) channels and results in calcium influx that triggers the exocytosis of insulin granules. Oxygen is important to drive this heavily metabolic process and insulin secretion is significantly influenced by the dynamics of blood flow and oxygen supply in addition to glucose gradients. Islets readily perform this glucose-insulin response in vivo as they are highly perfused in the pancreas, each within one cell length from a capillary vessel. However, the dense network of intraislet capillaries is removed by collagenase during islet isolation2,3. Consequently, both oxygen and nutrient supplies are constrained to a 100 μm perimeter due to diffusion limitations.
Current techniques have limited success in recreating islet microenvironment
Recreating islet's native oxygen and glucose dynamics, key to modeling physiological and pathophysiological conditions, is difficult to achieve with standard hypoxic chambers that require elaborate flow and lack continuous monitoring of islet functions. Moreover, transplant therapies for Type I diabetes expose isolated islets to hypoxia in the hepatic portal system4 which has much lower pO2 (<2%, 5-15 mmHg) compared to physiological pancreas (5.6%, 40 mmHg). Post-transplant, the islet grafts take two weeks or more to be revascularized. It has been demonstrated that hypoxic exposure impairs islet's glucose-insulin coupling mechanism. Among the stimulus-secretion coupling factors, calcium signaling, mitochondrial potentials, and insulin kinetics can be easily monitored using microfluidics. Our previous microfluidic technique demonstrated this real-time monitoring with precise modulation of the aqueous microenvironment around single islet5,6. However, quantification of islet's hypoxic impairment is stymied by the lack of simultaneous stimulation and monitoring techniques. Therefore, combining microfluidic control of oxygen and islet monitoring can improve islet hypoxia studies.
Microfluidics can recreate and modulate the aqueous and oxygen microenvironment
The standard technique for tissue and culture hypoxia studies has been based on hypoxic chambers. In general, the hypoxic chambers provide single oxygen concentrations with equilibration times in ~10-30 min, incompatible with minute-scaled dynamic hypoxia. Two recent studies used small custom chambers for intermittent hypoxia exposure on whole mice, with conflicting results on glucose-induced insulin response7,8. Bear in mind that at the whole animal level, the respired oxygen is not directly translated to islet capillary pO2, due to controls in the respiratory system. Furthermore, these studies do not have standardized oxygen levels, nor do they provide real-time measures at the tissue level of islets.
On the other hand, oxygen microfluidics can surpass these limitations by controlling oxygen via gas channel networks. Moreover, microfluidics is compatible with live imaging during oxygen modulation, a feat currently not possible with standard hypoxic chambers. A number of these novel microfluidics approaches utilize the gas permeability of polydimethylsiloxane to dissolve oxygen concentrations into microchannels that flow media over target cells9-14. These devices have also integrated multiple discrete oxygen concentrations, fluorescence based oxygen sensors, and even chemical oxygen generation on-chip.
Liquid solvation-based microfluidics have a hard time maintaining stable, continuous gradients as it depends on convective mixing which is sensitive to flow conditions. In comparison, the technique we use here focuses on decreasing the diffusion path of oxygen delivery. The gas solvation and shear flow are eliminated by directly diffusing oxygen across a membrane seeded with cells or islet tissues. This removes the extra microfluidics required to control solvation and prevents unnecessary shear stress to the islets, which itself can trigger insulin release. This platform has been used to demonstrate reactive oxygen species (ROS) up-regulation at both hyperoxic and hypoxic extremes (2-97% O2) in cell culture1,15. Because of the direct delivery of oxygen and removal of shear flow, our diffusion-based platform provides the optimal microfluidic solution for studying islet hypoxia.
Multimodal stimulation and monitoring
Diffusion-based microfluidics also brings additional benefits when adapted for studying islet microphysiology. By using a membrane as a diffusion barrier, the liquid can be isolated from the oxygen modulations, enabling controls of aqueous glucose stimulations independently from hypoxic stimulations. This creates a sandwich-like simultaneous stimulation that spatially pin-points delivery to the islets. Furthermore, as the gas is temporally modulated via computerized microinjectors, we can modulate the oxygen concentration from 21-0% digitally with transient time less than 60 sec. The dynamic controls of the oxygen and glucose microenvironment at the microscope allow a real-time multimodal protocol that would not be possible or extraordinarily cumbersome using standard hypoxic chambers. Using this device, calcium signaling (Fura-AM), mitochondrial potentials (Rhodamine 123), and insulin kinetics (ELISA) were monitored to provide a complete picture of the dynamic glucose-insulin response under hypoxia.
1. Preparing the Mouse Islets
2. Making the Microfluidic Platform
3. Microdispenser Setup
4. Setting Up at the Microscopy
5. Running the Simultaneous Oxygen and Glucose Stimulation
Central to this islet hypoxia technique is the ability to modulate aqueous and gaseous phase stimulation in the same microfluidic chamber with minute-scale transients. Figure 1 is a representative result of the a) dual stimulations and b) fast modulations measured within the islet chamber. Aqueous modulation, shown by introduction of fluorescein into the chamber, achieves equilibrium in three to four minutes of mixing. Furthermore, oxygen can be stepped from 5-21% with fast transients, enabling cycling of oxygen with periods as short as 2 min. Different cycling depths and frequencies can also be achieved as shown in Figure 2.
When this cycling is applied to create intermittent hypoxia at the islets, one can observe the benefits of preconditioning islets against hypoxia, as compared to a regular, normoxic pulse, Figure 3a. Because intracellular calcium flux—the signaling mechanism of insulin secretion—is monitored in real-time, effects of hypoxia and IH can be observed in the overshoot and oscillation damping of calcium transients, Figure 3b. These are important parameters associated with KATP channels suggested to control the preconditioning process. Furthermore, mitochondria's link to metabolism and hypoxia can be visualized by monitoring mitochondrial potentials using Rh123. Finally, collection of microfluidic effluents allows ELISA assay of the total insulin quantity. Calcium, mitochondrial potential, and insulin are three parameters that begin to build a multimodal view of the glucose-insulin response under hypoxic transients, Figure 3c.
Figure 1. Simultaneous oxygen and glucose stimulations. (a) Static controls. Top: chamber introduction of FITC molecule at 250 μl/min stabilizes within 3 min of mixing time. Bottom: gas control provides stable delivery of 5, 10, and 21% oxygen at the membrane. (b) Temporal control. Cycling of oxygen between 5-21% is possible with 1 min period as measured both at the gas delivery (diffused) and surface of microwells (dissolved).
Figure 2. Microfluidic device can also generate other oxygen profiles. Different IH profiles can be obtained by varying the depth (5-10-15%) as well as the periods (3-6-1 min) of the cycling via gas mixing from the computerized microinjectors.
Figure 3. IH preconditioned islets have improved responses to hypoxia. (a) Representative overview of preconditioning using IH, totaling 30 min exposure at 5%, showing enhanced hypoxic response compared to normoxic pulse (same islet batch in a previous experiment). 10 more minutes of subsequent hypoxia still retains preconditioning. (b) Overlaid comparison of mean normoxic, hypoxic, and preconditioned hypoxic responses. Inset shows representative traces with recovery of oscillation behavior. (c) Multimodal Fura-2, insulin, and Rh123 responses for different oxygen and chemical conditions: 21% oxygen, 5% oxygen, preconditioning (P+5%), diazoxide (D+5%), and 5HD (5HD+P+5%). Diazoxide is consistent with preconditioning while 5HD negates the benefits of preconditioning by opening and blocking KATP channels, respectively. Two-tailed t-tests: 5% vs. 21%, 5% vs. P+5%, D+5% vs. 5HD+P+5%; *p<0.05, **p<0.01, ***p<0.001.
The multiple modalities integrated in this islet hypoxia technique present several points noted here for troubleshooting. First the isolated islets continue to degrade and disintegrate in culture due to digestive enzymes from acinar cells. Standardizing experiments to 1-2 days after islet isolation is thus critical in obtaining consistent results. Second, the aqueous flow was stopped during hypoxia and intermittent hypoxia to prevent convective clearance at the boundary between laminar flow and diffusion. This seems to limit the duration of islet preconditioning. Future integration of a gas exchange in the aqueous channel can eliminate this minor clearance while still allowing rapid gas modulations at the membrane. Third, while loading the islets, the aqueous tubing should be reconnected carefully in reverse order (outlet then inlet) to avoid trapping air bubbles. Lastly, future device can be augmented with a fanned-out microfluidic distributor, to help distribute the cluster of islets over the entire chamber, at bottom of which can be patterned with an array of trapper pockets. This microfluidic distribution in addition to the pocket array will help create a positional array of islets for high-throughput experiments.
Prior to this microfluidic islet hypoxia technique, the fastest intermittent hypoxia modulations were achieved in one to three minute cycles by using small custom hypoxic chambers with high flow of pressurized gas. However, these can only be used on whole animals and not at the single islet level. Besides the uncertainty of the actual hypoxia level achieved in the whole animals' pancreas (after respiratory equilibrium) there is also the inability to probe glucose-insulin response in real-time, well-controlled microenvironments. In comparison, both aqueous and gas stimulations are controlled to minute time-scales in our microfluidics. These modulations are also mounted directly at the microscope for multiparametric monitoring. Prior to our technique, repeatable and well-characterized islet precondition has not been achievable. Oxygen-sensitive ex vivo tissues such as islets are optimally suited to this microfluidic platform as their microscaled dimensions (i.e. 100 μm radius) are trapped between smaller cell-culture platform and larger chamber apparatus. Beyond islets, a number of ex vivo tissues—including cardiac tissue, brain slices, and embryos—can be investigated using this technique.
The authors have nothing to disclose.
This work was supported by the National Institutes of Health Grants R01 DK091526 (JO), NSF 0852416(DTE), and Chicago Diabetes Project.
Reagent/Material | |||
Spinner | Laurell | WS-400 | |
SU8 | MicroChem | SU8-2150/SU8-2100 | |
Digital Hotplate | PMC Dataplate | 722A | |
UV Curing Lamp | OmniCure | S1000 | |
PMDS | Dow Chemical | Sylgard 184 | |
Corona Wand | ETP | BD-20AC | |
Vacuum Chamber | Bel-Art | 420220000 | |
Microdispensers | The Lee Company | IKTX0322000A | |
5 V and 20 V DC Power | Radio Shack | ||
NI USB | National Instrument | NI USB-6501 | |
Thermometer | Omega Engineering, Inc. | ||
Peristaltic Pump | Gilson | Minipulse 2 | |
Oxygen Sensor | Ocean Optics | NeoFox | |
Fraction Collector | Gilson | 203 | |
Pippette | Fisher Scientific | Finnpipette II 100μl | |
Inverted Epifluorescence Microscope | Leica | DMI 4000B | |
50 ml Conical Tubes | Fisher Scientific | ||
Fura-2 Fluorescence Dye | Molecular Probes, Life Technologies | ||
Rhodamine 123 Fluorescence Dye | Molecular Probes, Life Technologies | ||
Culture Media | Sigma-Aldrich | RPMI-1640 | |
HEPES | Sigma-Aldrich | ||
Glucose | Sigma-Aldrich | ||
Bovine Serum Albumin | Sigma-Aldrich | ||
30 in Silicone Tubings | Cole-Parmer | 1/16 in x 1/8 in | |
1.5 ml Eppendorf Tubes | Fisher Scientific | ||
Y-connectors | Cole-Parmer | 1/16 in and 4 mm | |
Syringe Connectors | Cole-Parmer | female Luer plug 1/16 in | |
Straight Connectors | Cole-Parmer | 1/16 in | |
Elbow Connector | Cole-Parmer | 1/16 in |