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Logo of nihpaAbout Author manuscriptsSubmit a manuscriptNIH Public Access; Author Manuscript; Accepted for publication in peer reviewed journal;
 
Nat Methods. Author manuscript; available in PMC Feb 1, 2011.
Published in final edited form as:
PMCID: PMC2941625
NIHMSID: NIHMS216983
High-throughput in vivo vertebrate screening
Carlos Pardo-Martin,1,2,3,5 Tsung-Yao Chang,1,5 Bryan Kyo Koo,1 Cody L. Gilleland,1 Steven C. Wasserman,4 and Mehmet Fatih Yanik1,4*
1Department of Electrical Engineering and Computer Science, Massachusetts Institute of Technology (MIT), Cambridge, MA 02139.
2School of Engineering and Applied Sciences, Harvard, Cambridge, MA 02138.
3Division of Health Sciences and Technology, MIT, Cambridge, MA 02139.
4Department of Biological Engineering, MIT, Cambridge, MA 02139.
* correspondence: yanik/at/mit.edu
5Equally contributing authors.
AUTHOR CONTRIBUTIONS CP-M, T-YC, SCW, and MFY designed the experiments and wrote the manuscript. CP-M, T-YC, BKK, and CLG performed the experiments.
Abstract
We demonstrate a high-throughput platform for cellular-resolution in vivo pharmaceutical and genetic screens on zebrafish larvae. The system automatically loads animals from reservoirs or multiwell plates, and positions and orients them for high-speed confocal imaging and laser manipulation of both superficial and deep organs within 19 seconds without damage. We show small-scale test screening of retinal axon guidance mutants and neuronal regeneration assays in combination with femtosecond laser microsurgery.
Small size, optical transparency of complex organs, and ease of culture make the zebrafish (Danio Rerio) larva an ideal organism for large-scale in vivo genetic and chemical studies of many processes that cannot be replicated in vitro. Zebrafish models of several human diseases have been developed1-5. Lead compounds discovered by screening chemical compound libraries for efficacy in zebrafish disease models have been useful for pharmaceutical discovery due to the high level of conservation of drug activity between mammals and zebrafish1-5.
Visualizing most zebrafish organs requires manipulating and properly orienting the animals. Even with confocal or two-photon microscopy, optical access is often impeded by pigmentation, by intervening organs such as eyes and heart, or by the highly autofluorescent yolk sac. Current methods to address these challenges involve treatment with the toxic chemical phenylthiourea to suppress pigmentation6, manually transferring animals from multiwell plates or reservoirs, and manually orienting them in viscous media such as agar. These processes are too slow and unreliable for high-throughput screens To improve the throughput and complexity of zebrafish screens, we developed the vertebrate automated screening technology (VAST) that automatically manipulates and images animals on the fly, eliminating the need for any manual handling (Fig. 1 and Online Methods).
Figure 1
Figure 1
Schematic of zebrafish manipulation and imaging platform. Larvae are automatically loaded to the system from either reservoirs or multi-well plates. Reservoirs are connected to the system via fluidic valves and a bubble mixer prevents the larvae from (more ...)
Each cycle of VAST includes the following steps: loading, detection, positioning, orienting, focusing, imaging, laser manipulation, and dispensing. Such an automated system makes both genetic and pharmaceutical whole-organism screens possible7 (Supplementary Fig. 1). During loading, the system extracts larvae either from a multiwell plate or a reservoir. A high-speed photodetection system composed of a photodiode and two LEDs discerns the entry of larvae into the loading tube. The photodiode senses transmitted light from one LED and scattered light from the other LED. By simultaneously monitoring both the transmission and scattering signals, the system discriminates larva from air bubbles and debris with 100% reliability (n = 1000). After loading and photodetection, the larva moves from the larger loading tube into a capillary8,9 positioned within the field-of-view (FOV) of an optical imaging and manipulation system. The capillary has a refractive index similar to water, allowing the use of high numerical-aperture (NA) water-immersion objectives that require short working distances. Using a fast camera and an automated image processing algorithm, the larva is coarsely positioned by the syringe pump. Next, a 3-axis stage automatically moves the capillary assembly to precisely position the larva’s head at the center of the FOV. The larva is then rotationally oriented by a pair of stepper motors. Thus, larvae can be arbitrarily positioned and oriented. In addition, larvae can be automatically re-oriented, thus allowing visualization of organs from multiple angles. At the end of the cycle, animals can be dispensed back into either individual wells or larger containers by executing the loading process in reverse. See Online Methods and Supplementary Fig. 2.
Larvae are imaged through two objective lenses: an upright, high-resolution water-immersion objective and an inverted air objective. This allows both wide-field fluorescence imaging and high-resolution confocal microscopy. Imaging most phenotypes requires larvae to be oriented at specific angles. For instance, the midline crossing of the Mauthner motor neuron axons that project into spinal cord is only visible when directly observed from the hindbrain (Fig 2a, 0°). At less favorable orientations, the structure is obscured. We performed a small-scale test screen on a similar phenotype – the midline crossing of retinal axon projections to the optic tectum (Fig. 2b and Supplementary Fig. 3). Screening for retinal axon misguidance mutants had previously led to the discovery of astray mutation in robo2 gene10. Homozygous astray (ast/ast) zebrafish fail to exhibit proper midline crossing, while the projections are normal in heterozygous (ast/+) zebrafish. Using our system, we were able to distinguish wild type larvae from robo2 mutants11 with a sensitivity of 100% and specificity of 98.8% for a 96-well plate with 83 randomly seeded mutants. The 1.20% false negative error in identification of ast/ast animals was due to the rare cases of mutants with strong phenotypic similarity to wild type. The system could thus be used for large-scale chemical screens for small molecules that rescue such misguidance.
Figure 2
Figure 2
Orientation, imaging, and screening of zebrafish larvae. (a) Schematic (left) showing the midline crossing of Mauthner axons. Right panels show confocal images of EGFP-expressing Mauthner cells at 0° and 15°. Magnified versions of marked (more ...)
In conjunction with sample positioning and orientation, VAST also allows in vivo optical manipulations such as localized activation of fluorescent reporters and ion channels, uncaging of compounds, and femtosecond laser microsurgery12 with subcellular precision. We illustrate the use of the system to study neuronal regeneration13 following injury by laser microsurgery14 (Fig. 3a). The lateral-neuron axon fiber bundle projecting along the trunk of a larva is visible when the larva is laterally oriented. The bundle is axotomized by focusing near-infrared femtosecond laser pulses on it. This process is semi-automated15: The user selects a cell body by clicking on a graphical user interface. An algorithm measures the user-specified distance from the cell body to the point of axotomy along the axon and the position stage automatically moves the selected axonal region to the focal spot of the laser for axotomy. The regenerating axonal fibers are shown at 18 and 24 hours post-axotomy in Fig. 3a. The laser pulses are delivered with high precision (1.7 μm)12, and the subsequent response of the tissue to the laser (i.e. immediate retraction of nerve fibers) show some variability, leading to a distribution of cut sizes (8.1 ± 5.5 μm, n = 30, ±s.d.) (Fig. 3b). 100% of the animals recovered from surgery within 30 minutes with no apparent morphological abnormality, and 100% of the animals survived 24 hours post surgery (n =30).
Figure 3
Figure 3
Laser microsurgery and neuronal regeneration. (a) Wide-field fluorescence images of GFP-expressing lateral-neuron axon fibres in a 3dpf larva are shown at the indicated times pre- and post- axotomy. (b) The distribution of laser cut sizes is shown (n (more ...)
A complete cycle of loading, positioning, cellular-resolution imaging, and dispensing an animal takes less than 16 seconds (Table 1). Axotomy requires an additional 2 seconds. Screening an entire multiwell plate took 31.85 minutes with an average of 19.9 seconds per well, which includes the additional interval for retracting, moving and inserting the loading apparatus, and sealing the wells. Animals can be loaded and imaged multiple times for time-lapse assays. Performed manually, assays of similar complexity require about 10 minutes per animal, and the assays are error-prone.
Table 1
Table 1
Average duration of screening steps
Zebrafish larvae are delicate and particularly susceptible to injury by tearing at sharp edges or by deformation. The most significant potential for damaging larvae occurs as they enter the loading tube at the high aspiration rates needed to achieve the desired throughput. To lessen this risk, the flow is started at a low initial rate and increased at an acceleration of 42 μl·s−2 until a larva is detected by the high-speed photodetector. The maximum flow rate is limited to 330 μl·s−1. At this maximum rate, no injury occurs while larvae are traveling within the tubing. After a larva is detected by the photodetector, the control software decreases the aspiration rate to 83 μl·s−1 to allow automated recognition by the camera.
We assessed the health of 450 larvae screened at 2 dpf at three different initial aspiration rates (Fig. 4a). The assessment was based on both functional and morphological criteria. At all flow rates, heartbeat and touch response matched those of controls. Tearing of yolk was never observed (n = 450). At the highest initial flow rate of 330 μl·s−1, 2.0% of the animals exhibited morphological abnormality. With a slightly slower initial aspiration rate (increasing the screening time by approximately 1 second), all health criteria matched those of controls (Fig. 4a). Post-manipulation developmental delay was measured by monitoring the time of appearance of the swimming bladder. There was no significant difference (One way ANOVA, P = 0.94, 3 independent experiments with n = 50 for each group) between the development of larvae that were manipulated by the system and control animals, even at the highest flow rates (Fig. 4b). Among the different larval age groups tested (i.e. 2-7 dpf, n > 100 per age), no difference in health assessment was observed.
Figure 4
Figure 4
Quantitative assessment of animal health. (a) Survival and abnormality of larvae as a function of initial flow rate (n = 150 for each rate). (b) Appearance time of swimming bladder in screened and control fish (n = 50).
In summary, we demonstrate a high-throughput vertebrate screening platform with cellular-resolution imaging and manipulation capabilities that should permit large-scale in vivo study of complex processes such as organ development, neural degeneration and regeneration, stem cell proliferation, cardiovascular, immune, endocrine, and nervous system functions, pathogenesis, cancer, and tissue specificity and toxicity of drugs.
High-throughput screening platform
The system can load larvae from reservoirs or multiwell plates (Fig. 1). The multiwell plate loading stage consists of 3 linear precision motors (RCA2, Intelligent Actuators). The motors are controlled by RACON 20/30 drivers (Intelligent Actuators). The loading head consists of a larva-loading and a water-supply metal tube with inner diameters of 1.0 and 0.2 mm, respectively (New England Small Tubing Inc.) inserted into a silicone rubber block. The silicon rubber block is pressed (by the loading stage motor) against the top of the multiwell plate to seal the wells. One tube aspirates the larva from the sealed well while the other tube injects water. Two fluidic valves (075P2NC12, Bio-Chem Fluidics) are used to switch the flow between the reservoirs and multiwell plate by pinching the silicone tubing (1/32″ ID × 3/32″ OD, Bio-Chem Fluidics). Larvae are driven through the system using a syringe pump (Carvo XLP6000, Tecan Systems). The photodetection system consists of a photodiode IC (OPT301, Texas Instruments) and two LEDs (Cree Inc) aligned in transmission and reflection configurations as shown. The photodiode IC contains an integrated amplifier. The imaging system consists of a dual (upright/inverted) microscope (Eclipse Ti, Nikon (inverted), Nikon 90i Digital Imaging Head (upright)) with two light sources (Mercury lamp, Nikon). The top port of the upright microcsope is equipped with a multi-beam laser confocal scanning head (Infinity 3, VisiTech) with a 1004 × 1002 pixel EMCCD camera (iXon+885, Andor Technology) for high-speed confocal imaging. For high-speed image sectioning, a piezo actuator with 400 μm travel distance (P-725 PIFOC, Physik Instrumente) holds either a 10× (NA = 0.5), 16× (NA = 0.8), or 20× (NA = 1.0) water immersion lens (Nikon). A high-speed CCD camera (GX-1050, Prosilica) is connected to the inverted microscope equipped with 10× air objective lens for larva detection, position, and rotation. Two precision stepping motors (KP35FM2-044, Japan Servo Co.) hold a capillary of diameter 800 μm along its axis of rotation. The motors are controlled by a microstepping driver (BSD-02LH, Interinar Electronics). The motor and capillary assembly is mounted on a 3-axis precision stage (MP-200, Sutter Instrument) with 0.04 μm resolution along each axis. Two NiDAQ input/output data cards (PCI-6512 and PCI-6259, National Instrument) installed in a DELL OptiPlex computer control the fluidic valves, stepping motors, and read out the voltage across the photodetector.
System automation
The detailed algorithm for operation sequence of the system is shown in the flowchart of Supplementary Figure 2. The system starts by initializing syringe pumps, cameras, lamps, shutters, position stages, and motors. The fluidic valves (Fig. 1) are switched to the source of fish i.e. either multiwell plate or fish reservoir. The larva is aspirated from the selected source at a constant rate of acceleration of 42 μl s−2 up to a maximum speed of 330 μl s−1. The photodetector is continuously sampled at 2 kHz rate via the NiDAQ PCI-6259 card until the intensity reading crosses a pre-determined threshold (the value of threshold is calibrated in advance by trial and error). Upon detection of the larva the fluidic valve is switched to the water reservoir if the larva is being loaded from the fish reservoir. The aspiration rate is subsequently decreased to 83 μl s−1 to avoid damaging the larva at the entrance of the capillary. The high-speed CCD at the bottom port continuously reads at 100 frames s−1. The pixel intensity is averaged over the entire field-of-view, and compared to a pre-determined threshold (value of threshold is calibrated in advance by trial and error). When average pixel intensity drops below the threshold, the aspiration is stopped. The capillary is then rotated via the motors until the larva is at the desired orientation. A large field-of-view image of the gross morphology of the larva is acquired by the CCD at the bottom port. The motorized shutter of the inverted microscope (i.e. bottom shutter) is closed while that of upright microscope (top shutter) is opened. Image acquisition is switched from the bottom CCD to either the top CCD or the high-speed scanning confocal head equipped with the EMCCD. Guided by fluorescence imaging, the region of interest is located. Either confocal stacks or wide-field fluorescence images are acquired. The top shutter is closed, and the bottom shutter opened. The image acquisition is switched to the bottom port. The system is now ready for the next cycle of operation. The control software is written in Matlab. The most recent version of the software is available upon request from the authors (MF Yanik, yanik/at/mit.edu).
Animals
The fluorescent retinal ganglion line (astrayti272z with brn3c:gap43-gfp), the fluorescent lateral neuron line, and the fluorescent mauthner line (ETj1282b:GFP) were maintained and crossed using standard techniques. All animal experiments were approved by MIT’s Committee on Animal Care under protocol numbered 0309-025-12.
Axon guidance screen
Genotypically homozygous +/+ and ast/ast fish were crossed to generate ast/+ larvae. A 96-well plate was randomly and partially populated with the heterozygous ast/+ progeny. The rest of the wells were populated with the homozygous progeny of ast/ast fish. A blind screen was performed by loading the animals from multi-well plates and orienting them to visualize midline crossing as in part (a) by a 10× (NA = 0.5) objective lens with long depth-of-focus in wide-field fluorescence imaging mode. Animals were blindly classified according to the observed phenotype.
Laser axotomy
A tunable femto-second laser (Mai Tai, Spectra-Physics Lasers) is guided to the upright microscope for laser axotomy as we previously described20. The axon fiber of GFP-expressing lateral neuron is cut 850 μm distance from the soma using ultrashort laser pulses with 780 nm wavelength, 100 fs duration, 12.7 nJ pulse energy, 80 MHz repetition rate, and 10 ms long pulse train focused by a 20× (NA = 1.0) objective lens. Statistics of laser cut sizes were quantified with 40× (NA = 0.8) objective lens. Surgeries were repeated on n = 30 animals with 100% success rate.
Assessment of animal health
The syringe was operated at three different initial aspiration rates of 165, 250, and 330 μl·s−1 for loading 2 dpf larvae from multiwells. n = 450 larvae in total were anesthetized with 0.20 mg·ml−1 Tricaine, loaded, and dispensed from the platform. A control group of n = 150 larvae from the same breed were similarly anesthetized. Health assessment was based on both functional and morphological criteria measured at t = 0, 12, 16, 20, 24, 28, 32 and 36 hours post screening. Functional criteria included visual confirmation of normal heartbeat, and reflex response to touch stimuli. Morphology criteria included bending (i.e. lordosis, kyphosis, and scoliosis) and craniofacial abnormalities. The criteria included those injuries even if the animals regenerated later.
Supplementary Material
supp info
ACKNOWLEDGMENTS
We thank the following funding sources: NIH Director’s Innovator Award (1-DP2-OD002989–01), Packard Award in Science and Engineering, Alfred P. Sloan Award, Sparc Grant from Broad Institute, National Science Foundation Fellowship, Foxconn Sponsorship, and the “LaCaixa” Graduate Fellowship. We also thank A. Amsterdam and N. Hopkins of MIT, A. Schier and I. Woods of Harvard University for the fluorescent lateral neuron line, C. Chien of the University of Utah for the fluorescent retinal ganglion line (astrayti272z with brn3c:gap43-gfp)10,11, S. Johnson from Washington University at St. Louis, and R. Jain and M. Granato of University of Pennsylvania for the fluorescent mauthner line (ETj1282b:GFP).
Footnotes
COMPETING INTERESTS STATEMENT Authors have two pending patents. MFY is founder and chief scientific advisor of Entera Pharmaceuticals.
1. Lieschke GJ, Currie PD. Animal models of human disease: zebrafish swim into view. Nat Rev Genet. 2007;8(5):353–67. [PubMed]
2. Zon LI, Peterson RT. In vivo drug discovery in the zebrafish. Nat Rev Drug Discovery. 2005;4(1):35–44. [PubMed]
3. Rubinstein AL. Zebrafish: from disease modeling to drug discovery. Curr Opin Drug Discov Devel. 2003;6(2):218–23. [PubMed]
4. McGrath P, Li C. Zebrafish: a predictive model for assessing drug-induced toxicity. Drug Discovery Today. 2008;13(9-10):394–401. [PubMed]
5. Shin JT, Fishman MC. From Zebrafish to human: modular medical models. Annu. Rev. Genomics. Hum. Genet. 2002;3:311–40. [PubMed]
6. Karlsson J, Hofsten JV, Olsson PE. Generating Transparent Zebrafish: A Refined Method to Improve Detection of Gene Expression During Embryonic Development. Marine Biotech. 2001;3:522–7. [PubMed]
7. Rohde CB, et al. Microfluidic system for on-chip high-throughput whole-animal sorting and screening at subcellular resolution. PNAS. 2007;104(35):13891–5. [PubMed]
8. Funfak A, Brosing A, Brand M, Kohler JM. Micro fluid segment technique for screening and development studies on Danio rerio embryos. Lab Chip. 2007;7:1132–8. [PubMed]
9. Buckley, et al. Zebrafish myelination: a transparent model for remyelination? Disease Models & Mechanisms. 2008;1:221–8. [PubMed]
10. Fricke C, et al. astray, a Zebrafish Homolog Required for Retinal Axon Guidance. Science. 2001;292:507–10. [PubMed]
11. Xiao T, Roeser T, Staub W, Baier H. A GFP-based genetic screen reveals mutations that disrupt the architecture of the zebrafish retinotectal projection. Development. 2005;132:2955–67. [PubMed]
12. Steinmeyer JD, Gilleland CL, Pardo-Martin C, Angel M, Rohde CB, Scott MA, Yanik MF. Construction of a femtosecond laser microsurgery system. Nature Protocol. 2010;5(3):395–407. [PubMed]
13. Bhatt DH, Otto SJ, Depoister B, Fetcho JR. Cyclic AMP-Induced Repair of Zebrafish Spinal Circuits. Nature. 2004;305:254–8. [PubMed]
14. Yanik MF, Cinar H, Cinar N, Chisholm A, Jin Y, Yakar AB. Neurosurgery: Functional regeneration after laser axotomy. Nature. 2004;432:822. [PubMed]
15. Zeng F, Rohde CB, Yanik MF. Subcellular precision on-chip small-animal immobilization, multi-photon imaging and femtosecond-laser manipulation. Lab Chip. 2008;8:653–6. [PubMed]