Using Zebrafish Larvae to Study the Pathological Consequences of Hemorrhagic Stroke

Siobhan Crilly; Alexandra Njegic; Adrian R. Parry-Jones; Stuart M. Allan; Paul R. Kasher

doi:10.3791/59716

JoVE Journal > Neuroscience

Neurosciences

Using Zebrafish Larvae to Study the Pathological Consequences of Hemorrhagic Stroke

Published: June 05, 2019

doi:

10.3791/59716

Siobhan Crilly¹, Alexandra Njegic², Adrian R. Parry-Jones^2,3, Stuart M. Allan^1,3, Paul R. Kasher^1,3

¹Division of Neuroscience and Experimental Psychology, School of Biological Sciences, Manchester Academic Health Science Centre,University of Manchester, ²Division of Cardiovascular Sciences, School of Medical Sciences, Faculty of Biology, Medicine and Health, Manchester Academic Health Science Centre,University of Manchester, ³Lydia Becker Institute of Immunology and Inflammation,University of Manchester

Summary

Here we present a protocol to quantify brain injury, locomotor deficits and neuroinflammation following bleeding in the brain in zebrafish larvae, in the context of human intracerebral hemorrhage (ICH).

Abstract

Despite being the most severe subtype of stroke with high global mortality, there is no specific treatment for patients with intracerebral hemorrhage (ICH). Modelling ICH pre-clinically has proven difficult, and current rodent models poorly recapitulate the spontaneous nature of human ICH. Therefore, there is an urgent requirement for alternative pre-clinical methodologies for study of disease mechanisms in ICH and for potential drug discovery.

The use of zebrafish represents an increasingly popular approach for translational research, primarily due to a number of advantages they possess over mammalian models of disease, including prolific reproduction rates and larval transparency allowing for live imaging. Other groups have established that zebrafish larvae can exhibit spontaneous ICH following genetic or chemical disruption of cerebrovascular development. The aim of this methodology is to utilize such models to study the pathological consequences of brain hemorrhage, in the context of pre-clinical ICH research. By using live imaging and motility assays, brain damage, neuroinflammation and locomotor function following ICH can be assessed and quantified.

This study shows that key pathological consequences of brain hemorrhage in humans are conserved in zebrafish larvae highlighting the model organism as a valuable in vivo system for pre-clinical investigation of ICH. The aim of this methodology is to enable the pre-clinical stroke community to employ the zebrafish larval model as an alternative complementary model system to rodents.

Introduction

Intracerebral hemorrhage (ICH) is the most severe sub-type of stroke associated with spontaneous cerebral vessel rupture and bleeding into the parenchyma leading to brain damage, physical disability and often death¹. Despite the high mortality and morbidity rate associated with ICH², understanding of the underpinning etiology and post-hemorrhage pathology is still lacking. As such, there are no specific treatments to prevent ICH or improve patient outcomes. Most of our understanding of disease biology has come from pre-clinical rodent models of ICH³, however studies to-date in these models have failed to translate any successful therapeutic to the clinic⁴^,⁵. This failure may be due in part, to some limitations of these preclinical models, including the inability to easily recapitulate the spontaneous nature of human disease and the requirement for invasive surgery to generate the models in mammals⁶. Additionally, rodents pose practical problems with regards to observing the rapid onset of cellular responses to ICH in intact tissue. Given the lack of translation from rodent models, developing alternative models of spontaneous ICH is imperative if we are to overcome these practical problems and help identify novel drug targets.

The molecular mechanisms of vascular development are well conserved amongst vertebrates including zebrafish (Danio rerio)⁷. As such, the adoption of this model organism is becoming an ever more useful mechanistic strategy for studying cerebrovascular disease⁸. A number of zebrafish models have been generated which recapitulate phenotypes associated with stroke-related conditions⁹^,¹⁰^,¹¹^,¹². The use of zebrafish larvae to investigate disease pathogenesis offers both practical and scientific advantages over mammalian models⁸. This includes high reproduction rates, rapid development and larval transparency that allows for intravital imaging without the invasive constraints associated with rodents. Coupling these advantages with the wide range of transgenic reporter lines available within the zebrafish research community amounts to a powerful in vivo approach for studying disease biology, not yet utilized for studying the pathological consequences of ICH.

The injury response to blood in the brain is biphasic¹³; the primary insult causes neuronal death and cell necrosis, which then initiates a secondary wave of damage that is induced by innate immune activation. The second phase of brain injury, in particular the neuroinflammatory component, is considered a realistic target for future drug treatment¹³. Spontaneous and cerebral-specific hemorrhages have been described in zebrafish larvae previously¹⁴^,¹⁵^,¹⁶^,¹⁷^,¹⁸^,¹⁹. Two such models are the use of atorvastatin (ATV) at 24 h post-fertilization (hpf) to inhibit the HMGCR pathway and cholesterol biosynthesis¹⁴, and a bubblehead (bbh) mutant which express a hypomorphic mutation in the arhgef7 gene, βpix, and subsequently inhibits actin remodeling for tight endovascular junctions¹⁸. These models exhibit spontaneous cerebral-specific blood vessel rupture at the onset of circulation (~33 hpf). Recently, we have characterized these models further to reveal that key aspects of the brain injury response is conserved between humans and zebrafish larvae²⁰. This study demonstrates the methodology required to obtain and visualize spontaneous brain hemorrhages in zebrafish larvae and how to quantify brain injury, and locomotor and neuroinflammatory phenotypes that relate to the human condition. These data and techniques support the use of this model species as a valuable complementary system for pre-clinical ICH research.

Protocol

Zebrafish were raised and maintained at The University of Manchester Biological Services Unit under standard conditions as previously described²¹. Adult zebrafish husbandry was approved by the University of Manchester Animal Welfare and Ethical Review Board. All experiments were performed in accordance with U.K. Home Office regulations (PPL:P132EB6D7).

NOTE: Transgenic lines used in this study include macrophage-specific lineage mpeg1:mCherry (constructed in-house as previously described²²), neutrophil-specific mpo:GFP²³,erythroid-specific gata1:dsRed²⁴ and ubiq:secAnnexinV-mVenus, a reporter for cell death (re-derived in house²⁵)on wild-type, nacre (mitfa^w2/w2) and mutant (bbh^m292) backgrounds. Figure 1 shows the experimental timeline.

Figure 1: Graphic of experimental timeline to characterize brain injury, locomotor and neuroinflammatory outcomes. ICH, intracerebral hemorrhage; bbh, bubblehead. Figure has been reproduced from Crilly et al.²⁰ with permission under a Creative Commons license. Please click here to view a larger version of this figure.

1. Day 0: Egg production and collection

Collect fertilized embryos from natural spawning in breeding boxes produced from 1 male and 1-2 female adult zebrafish.
NOTE: For atorvastatin protocol any wildtype/transgenic animals can be used however hemorrhage rates differ slightly between strains.
Incubate 100 embryos at 28 °C in standard E3 embryo medium per Petri dish and stage according to standard guidelines²⁶.
At ~6 hours post fertilization (hpf) remove dead and unfertilized embryos from the dish using a Pasteur pipette.

2. Day 1: Atorvastatin treatment at 24 hpf

Dechorionate embryos for atorvastatin treatment using sharp ultra thin dissection forceps²⁷. Numbers required for experimentation can be adjusted accordingly.
Add 30 mL of E3 embryo medium to two clean Petri dishes. Use one dish for 100 embryos.
NOTE: If plates are designed for cell culture, dechorionated zebrafish at this early stage often stick to the bottom. To avoid this, rinse the plates thoroughly in clean water before use.
Remove 60 µL of embryo water from the treatment plate and add 60 µL of 0.5 mM atorvastatin (ATV). At a 0.5 mM stock concentration, the above dilution will result in a final concentration of 1 µM which will result in ~20% of larvae non-hemorrhaged (ICH-) and ~80% of larvae hemorrhaged (ICH+). Use the other plate for untreated controls
NOTE: Atorvastatin is solubilized in distilled water (3 mg into 10 mL) to make a 0.5 mM stock solution. Incubate overnight at room temperature in the dark with agitation as solubilization takes some time. Complete solubilization can take up to 1 week. Do not use DMSO. Solution is aliquoted and stored at -20°C. Do not freeze thaw.
Using a Pasteur pipette, transfer 100 embryos in as little water as possible to the treatment plates.
Incubate the plates at 28 °C.
NOTE: ICH will occur between 33 and 48 hpf. Atorvastatin does not need to be removed as incubation longer than 24 h does not cause any further developmental issues.

3. Day 2: Separating ICH- and ICH+ populations at 50 hpf

Separate ICH+ fish from ICH- populations and transfer to new dishes for ease.
1. If using the ATV model at a concentration of 1 µM, 75-100% of larvae will exhibit hemorrhage (ICH+) at this time point.
  NOTE: The response of the larvae differs between strains, if larvae are not hemorrhaging at the desired frequencies, use a fresh batch of atorvastatin or a higher concentration. If larvae have not exhibited hemorrhage by 48 hpf then consider them ICH-.
2. If using the bbh model, all homozygous mutants will exhibit hemorrhage by 48 hpf. If using a heterozygous incross, the ICH- heterozygous and wildtype siblings can be used as control animals for experiments.
If necessary, anaesthetize the larvae by adding 0.02% MS222 to the E3 media. Using a Pasteur pipette, sort the larvae for presence of blood in the head into fresh E3 media. See Figure 2.
NOTE: Blood in the head may appear in the fore, mid or hindbrain or in combination, and bleed volume can vary between animals. In the bbh mutants, ICH is often associated with severe edema recognizable by larger heads, wider space between the eyes and a more diffuse bleed. However not all ICH+ bbh larvae exhibit edema.

Figure 2: ICH+ brain hemorrhage phenotypes. Examples of larval ICH phenotypes maintained on a transgenic gata1:DsRed reporter nacre background observed with a brightfield stereomicroscope (top panels) and fluorescence (bottom panel) at ~48 h post-fertilization. No hemorrhages were observed in ICH-larvae (left panels). A distinct accumulation of red blood cells in the forebrain and hindbrain (arrows) were observed in ICH+ larvae (right panels). Scale bars represent 250 µm. Figure has been reproduced from Crilly et al.²⁰ with permission under a Creative Commons license. Please click here to view a larger version of this figure.

4. Day 3: Cell death and leukocyte analysis at 72 hpf

Screen the larvae using a fluorescence microscope to ensure the expression of fluorescent protein.
NOTE: In this study, transgenic ubiq:secAnnexinV-mVenus larvae were used to report brain cell death and double transgenic mpo:GFP;mpeg1:mCherry or ubiq:secAnnexinV-mVenus;mpeg1:mCherry used for leukocyte analysis.
Fill the lightsheet mounting chamber with E3 media containing 0.02% MS222.
Anaesthetize the larvae using 0.02% MS222. Transfer larvae for mounting (n = 1-6) to a dry Petri dish surface in a single droplet. Remove as much liquid as possible.
NOTE: 1.5% low melt agarose is prepared using 0.15 g of low melt agarose dissolved in 10 mL of E3 medium without methylene blue in a microwave and kept at 45 °C until use.
Add a drop of 1.5% low-melt agarose (maintained as liquid in a 45 °C heat block) to the larvae and using a 800 µm mounting capillary, and draw the larvae up head first. If positioning is not accurate the larvae can be expelled from the agarose and mounted again. Leave the capillary to cool before inserting into the lightsheet chamber.
NOTE: Alternatively, a confocal microscope could be used for this procedure. For this, larvae should be mounted laterally in agarose on a glass bottom dish.
Acquire z-stack images of the head between the eye lenses (~300 µm) and process to maximum intensity projection image.
1. Analyze brain region from images collected for total number of fluorescent cells and total intensity fluorescence²⁰.
Create a time lapse video of multiple projection composites over 18-24 h to track leukocyte mobility and interaction with dying cells.
NOTE: If long term live imaging is performed, only one larva is mounted in the capillary.
When imaging is completed expel the larvae from the mounting capillary into a lethal overdose of 4% MS222 to euthanize.

5. Day 3: Selecting larvae for motility assay at 72 hpf

Anaesthetize larvae in the petri dishes with 0.02% MS222.
Randomly select n = 24 larvae for motility assay and transfer into fresh E3 media and allow animals to recover from anesthetic.
NOTE: Anesthetic at this point removes selection bias for slow swimmers that are easy to catch.

6. Day 3-5: Assaying locomotion at 72, 96 and 120 hpf

Transfer larvae selected at 72 hpf into E3 medium without methylene blue.
NOTE: For assaying at 3 dpf allow the larvae ample time to recover from anesthetic (>1 h).
Plate one larva in 1 mL per well of a 24-well plate using a pipette.
NOTE: Cut the end of the pipette tip to avoid damaging the larvae. Plate size can be changed according to experimental design.
Load plates into the camera chamber and assay motion for 10 min using a white light startle routine to increase spontaneous swimming.
NOTE: Swimming behavior was tracked using a camera chamber and tracking software (see the Table of Materials).
Repeat experiment with the same larvae at 96 and 120 hpf. Move larvae from individual housing in assay plate to a Petri dish and incubate at 28 °C in between assays.
At assay completion, euthanize larvae in a lethal overdose of 4% MS222.

Representative Results

Assessment of brain cell death using transgenic ubiq:secAnnexinV-mVenus results in clear definitive clusters of dying cells in ICH+ larvae in both ATV and bbh models that are absent in all ICH- larvae (Figure 3). Clusters recede before 96 hpf. Through image analysis, bleeding is associated with a significant two-fold increase in total intensity of fluorescence signal in the brain, indicating marked cell death.

A neuroinflammatory response is identified in ICH+ larvae by significantly increased numbers of mpeg1 positive macrophage cells in the brain. The number of total mpo positive neutrophil cells also increased however this did not reach statistical significance (Figure 4). The morphology of the mpeg1 positive macrophages can also be seen to change in ICH+ larvae as the cells adopt an active, rounded, amoeboid shape. These activated rounded cells can also be monitored over time to show an increased phagocytic response of the ubiq:secAnnexinV-mVenus expressing dying cells in ICH+ larvae (Figure 5). mpeg1 positive macrophages exhibiting ramified processes were categorized as inactive.

Brain hemorrhage is associated with a significant decrease in motility at 72 and 96 hpf in comparison to ICH- sibling controls in both bbh and ATV models (Figure 6). Motility at 120 hpf recovers to near baseline levels. There are often differences in baseline motility between egg clutches and strains and so comparison should be made to ICH- controls every time.

Figure 3: Intracerebral hemorrhage (ICH) in zebrafish larvae results in a quantifiable brain injury. (A) Representative images of the brain injury phenotype in ICH+ larvae (right panels), in comparison to ICH- siblings (left panels), at 72 hpf. Brightfield images (bottom panels, scale bar = 250 µm) demonstrate the presence of brain bleeds (arrows) in ICH+ larvae. Fluorescent microscopy was performed to visualize cell death in the ubiq:secAnnexinV-mVenus reporter line (top panels, scale bar = 100 µm). Clusters of dying cells were observed in peri-hematomal regions. Images were cropped to brain-only regions and analyzed for total green fluorescence intensity in round particles larger than 30 pixels in diameter (white line) using the macro in Supplementary File 1. (B) Quantification of fluorescence signal in the brains of untreated, ICH- and ICH+ larvae obtained through the ATV model (n = 12 per group; 3 independent replicates) at 72 hpf. Significant differences were observed when comparing ICH+ with untreated (**p = 0.004) and with ICH- (*p = 0.03) siblings. (C) Quantification of fluorescence signal as a read out for annexinV binding in the brains of ICH- and ICH+ larvae obtained through the bubblehead (bbh) model (n = 12 per group; 2 independent replicates) at 72 hpf. Graphs show SD from the mean. A significant difference in mVenus fluorescence was observed between ICH+ and ICH- age-matched siblings (**p = 0.002). Figure has been reproduced from Crilly et al.²⁰ with permission under a Creative Commons license. Please click here to view a larger version of this figure.

Figure 4: Intracerebral hemorrhage (ICH) initiates an innate cellular immune response in the zebrafish larval brain. Numbers of leukocytes quantified within the brain regions previously described for mpo:GFP;mpeg1:dsRed double transgenic larvae (n = 8 per group; 2 independent replicates) at 72 hpf reveals a significant increase in macrophages (*p = 0.01), but not neutrophils (p = 0.5), in response to ICH. Figure has been reproduced from Crilly et al.²⁰ with permission under a Creative Commons license. Please click here to view a larger version of this figure.

Figure 5: Activated macrophage cells show a phagocytic response to the brain lesion. (A) Representative time-lapse stills²⁰ showing a ramified patrolling macrophage migrating towards an annexinV positive cell (i – vi). Stills are obtained from a series of images taken of the whole brain using a 20x objective. Scale bar represents 50 µm. The macrophage acquired an amoeboid morphology (v) before phagocytosing the annexinV-positive cell (vi, vii). After phagocytosis the macrophage resumes a ramified morphology and migrates away and the annexinV-positive cell can no longer be seen (viii). Ramified macrophage (#), annexinV positive cell (arrow), amoeboid macrophage (*) are indicated. (B) Representative images of mpeg1-positive cells in the ICH- and ICH+ larval brain exhibiting amoeboid and ramified morphologies. Scale bars represent 50 µm. (C) An increased proportion of amoeboid (phagocytic) and decreased proportion of ramified (inactive) macrophages was observed in ICH+ brains in comparison to ICH- siblings. Figure has been reproduced from Crilly et al.²⁰ with permission under a Creative Commons license. Please click here to view a larger version of this figure.

Figure 6: ICH-induced brain injury results in a quantifiable locomotor deficit in zebrafish larvae. (A) Representative examples of the swimming tracks in ICH- and ICH+ bbh larvae at 72, 96 and 120 hpf. (B) ICH+ larvae exhibited a significant decrease in the cumulative time spent mobile during the 10 min recording period at both 72 and 96 hpf. Significance was lost at the 120 hpf time point potentially alluding to recovery from brain injury (n = 24 larvae per group; 3 independent replicates; ****p = 0.00006; **p = 0.003; ns: p = 0.08). (C) Quantification of cumulative time spent moving in untreated and ATV-treated ICH- and ICH+ larvae at 120 hpf. ICH+ larvae exhibited a significant decrease in the cumulative time spent mobile during the 10 min recording period. Three technical replicates (n = 24 larvae per group) were used to calculate SD from the mean (***p = 0.00004, **p = 0.0003). Figure has been reproduced from Crilly et al.²⁰ with permission under a Creative Commons license. Please click here to view a larger version of this figure.

Supplementary File 1. Please click here to download this file.

Discussion

This study shows that ICH in zebrafish larvae induces a brain injury response that recapitulates key aspects of the human condition that can be systematically assayed and quantified. Zebrafish offer a consistent and reproducible model of spontaneous ICH which will assist with future drug intervention studies focused on targeting blood-induced brain injury, rather than preventing vessel rupture¹⁷^,²⁸. Indeed, given the rapid nature of disease onset akin to the clinical situation, such an approach offers exciting prospects for successful translation in the future.

Some limitations are associated with the use of zebrafish larvae, such as the use of a developing system and taxonomic rank, however the practical and scientific advantages of this model must be considered to offer new insights into ICH. No surgery is required to initiate a haemorrhage or to monitor cellular processes over extended periods of time after injury. High fecundity of zebrafish pairings generate easily accessible and large sample sizes, and due to the fast development of the larvae the experimental timeline is significantly reduced compared to rodent studies²⁹^,³⁰.

Currently these models are fit to use for elucidating the immediate pathological and immunological response to spontaneous ICH in the brain of live intact animals. Potentially, this model can be adapted for medium-high throughput drug screens for ICH therapies, whether preventative or recovery promoting. As such, the post-ICH pathologies presented in this study represent an alternative, complementary platform for pre-clinical ICH research.

Divulgations

The authors have nothing to disclose.

Acknowledgements

We would like to thank Dr David Spiller and the University of Manchester Systems Microscopy Core Facility for use of the equipment, Prof. Richard Baines for the use of DanioVision and Dr. Jack Rivers-Auty for statistical consultation. The bbh line was kindly shared by Nicole Munsie from Dr. Sarah Child's lab at the University of Calgary. We also thank Prof. Stephen Renshaw, Dr. Adam Hurlstone, Dr. Andrew Badrock and Dr. Helen Young for fish lines and equipment.

This study was supported by the NC3Rs (NC/N002598/1), Stroke Association (TSA LECT 2017/02), ERA-NET NEURON (MR/M501803/1) and The British Heart Foundation (FS/15/67/32038). We are also particularly thankful to The Natalie Kate Moss Trust and the University of Manchester Faculty of Biology, Medicine and Health for their continued financial support.

Materials

24 well plates	Sigma-Aldrich	CLS3527
28 °C incubator	LMS	210
Atorvastatin	Sigma-Aldrich	PZ0001-5mg
Breeding boxes	Thoren Aquatics systems	10011
Daniovision observation chamber	Noldus	n/a
E3 medium 1x			4% Instant Ocean, 500 µL methylene blue in 1 L dH₂O
EthoVision XT software	Noldus	version 11
Heat block	Grant-Bio	PHMT-PSC18
Instant ocean	Instant Ocean	SS15-10
Lightsheet microscope	Zeiss	Z.1
Lightsheet microscope mounting capillary	Zeiss	402100-9320-000
Low melt agarose	Promega	V2111
Methylene Blue	Sigma-Aldrich	319112-100ML
Microscope	Leica	MZ95	dissection microscope
Microscope	Leica	M165FC	fluorescent microscope
MS222			4g tricaine powder, 500 mL of dH₂O, 10 mL of 1 M Tris (pH 9). Adjust pH to ~7
P1000 pipette	Gilson	F144059M
P1000 pipette tips	Starlab	S1122-1830
Pasteur pipettes	Starlab	E1414-0300
Petri dishes	Corning	101VR20
Pipetboy	Integra Biosciences	PIPETBOY
Stripette 25ml	Corning	CLS3527
Tricaine powder	Sigma-Aldrich	A5040-25G
Tris Base	Fisher BioReagents	BP152-1
Ultra fine dissection forceps	Agar scientific	AGT502
Zen software	Zeiss	version 2.3

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Crilly, S., Njegic, A., Parry-Jones, A. R., Allan, S. M., Kasher, P. R. Using Zebrafish Larvae to Study the Pathological Consequences of Hemorrhagic Stroke. J. Vis. Exp. (148), e59716, doi:10.3791/59716 (2019).