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VascuViz: a multimodality and multiscale imaging and visualization pipeline for vascular systems biology

Nature Methods volume 19, pages 242–254 (2022)Cite this article

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Abstract

Despite advances in imaging, image-based vascular systems biology has remained challenging because blood vessel data are often available only from a single modality or at a given spatial scale, and cross-modality data are difficult to integrate. Therefore, there is an exigent need for a multimodality pipeline that enables ex vivo vascular imaging with magnetic resonance imaging, computed tomography and optical microscopy of the same sample, while permitting imaging with complementary contrast mechanisms from the whole-organ to endothelial cell spatial scales. To achieve this, we developed ‘VascuViz’—an easy-to-use method for simultaneous three-dimensional imaging and visualization of the vascular microenvironment using magnetic resonance imaging, computed tomography and optical microscopy in the same intact, unsectioned tissue. The VascuViz workflow permits multimodal imaging with a single labeling step using commercial reagents and is compatible with diverse tissue types and protocols. VascuViz’s interdisciplinary utility in conjunction with new data visualization approaches opens up new vistas in image-based vascular systems biology.

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Fig. 1: Overview of the VascuViz pipeline for multimodality 3D vascular imaging and multiscale data integration.
Fig. 2: Concurrent imaging of GalRh–BVu bearing murine tissues with MRI, CT and optical contrast mechanisms.
Fig. 3: Multicontrast characterization of the VME in a human breast cancer model.
Fig. 4: Visualization of multimodality 3D data from the murine brain for multiscale neurovascular systems biology.
Fig. 5: Computationally generated hemodynamic contrast from VascuViz-derived 3D neurovascular data.
Fig. 6: Multimodality 3D mapping of the vasculature in the murine hind limb and kidney.

Data availability

The authors declare that all the data supporting the findings of this study are included in the paper and its Extended Data and supplementary information files. This includes the availability of imaging data for: (1) the murine brain in Figs. 4 and 5, Extended Data Figs. 5 and 7, Supplementary Tables 2 and 3 and Supplementary Video 1, (2) the breast tumor xenograft in Fig. 3 and Extended Data Figs. 2 and 3 and (3) the kidney and hind limb in Fig. 6. Finally, IHC and H&E data are available in Fig. 2 and Extended Data Fig. 1. The mouse hippocampal data that were used for the labeling of the cornu ammonis and dentate gyrus layers can be accessed freely from the Australian Mouse Brain Mapping Consortium (AMBMC) weblink: www.imaging.org.au/AMBMC.

Code availability

MATLAB code used in the paper will be made available upon reasonable request from the corresponding author.

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Acknowledgements

This work was supported by NIH/NCI grant nos. 51R01CA196701-05, 1R01CA237597-01A1 and 5R01DE027957-02 (A.P.P.); NIH Instrumentation grant no. S10OD012287 (Cornell University) and a Sidney Kimmel Comprehensive Cancer Center, Quantitative Sciences Pilot Project grant (A.B.). We thank D. Yang for assistance with Supplementary Video 1; Q. Wang for assistance with perfusion experiments; Z. Hou for assistance with image coregistration; A.S. Popel for providing the 4T1 tumor model and R. Pathak for assistance with data segmentation. This work is dedicated to the memories of S. Bhargava and P.I. Pathak.

Author information

Authors and Affiliations

  1. Russell H. Morgan Department of Radiology and Radiological Science, The Johns Hopkins University School of Medicine, Baltimore, MD, USA

    Akanksha Bhargava, Janaka Senarathna, Manisha Aggarwal & Arvind P. Pathak

  2. Biomedical Engineering, The Johns Hopkins University School of Medicine, Baltimore, MD, USA

    Benjamin Monteagudo, Yunke Ren & Arvind P. Pathak

  3. Departments of Orthopedic Surgery, The Johns Hopkins University School of Medicine, Baltimore, MD, USA

    Priyanka Kushwaha & Ryan C. Riddle

  4. Research and Development Service, Baltimore Veterans Administration Medical Center, Baltimore, MD, USA

    Ryan C. Riddle

  5. Electrical Engineering, The Johns Hopkins University, Baltimore, MD, USA

    Arvind P. Pathak

  6. The Sidney Kimmel Comprehensive Cancer Center, The Johns Hopkins University School of Medicine, Baltimore, MD, USA

    Arvind P. Pathak

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  1. Akanksha Bhargava
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Contributions

Conception and optimization of the GalRh–BVu polymer and study design were carried out by A.P.P. and A.B. Sample preparation and ex vivo MRI were conducted by A.B., M.A. and A.P.P. Sample preparation and ex vivo CT were carried out by A.B., P.K., R.C.R. and A.P.P. Sample preparation and ex vivo optical imaging were performed by A.B., B.M. and A.P.P. Sample preparation and IHC were carried out by A.B. and A.P.P. Sample preparation and in vivo imaging were performed by J.S., Y.R., A.B. and A.P.P. In vivo data analysis and data integration were carried out by A.B., J.S., Y.R. and A.P.P. Ex vivo data analysis, data integration and visualization were carried out by A.B., B.M. and A.P.P. The manuscript was prepared by A.B., M.A. and A.P.P. Results, discussion and data interpretation were carried out by all authors, along with input and revisions.

Corresponding author

Correspondence to Arvind P. Pathak.

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The authors declare no competing interests.

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Nature Methods thanks Shayne Peirce-Cottler and the other, anonymous, reviewer(s) for their contribution to the peer review of this work. Rita Strack was the primary editor on this article and managed its editorial process and peer review in collaboration with the rest of the editorial team.

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Extended data

Extended Data Fig. 1 The GalRh-BVu polymer did not interfere with histopathological workflows.

The GalRh-BVu polymer was compatible with H&E staining of paraffin-embedded (PE) tissues as shown for a 4T1 tumor xenograft sample (a-b), and a kidney sample (c-d). The intravascular polymer appeared dark brown on H&E images as seen in (b) the tumor rim vasculature from (a), and (d) renal cortex vasculature from (c). Black arrows point to a perfused glomerulus in (c-d). The polymer also did not interfere with H&E staining of frozen tissues as shown for the murine hippocampus (e) and cortex (f-g). In H&E labeled images, the cytoarchitecture of the hippocampus and cortex could also be complemented with the vascular visibility of the GalRh-BVu polymer (e-g). The GalRh-BVu polymer bearing blood vessels in (g) could also be imaged using fluorescence microscopy as shown in (h). Similarly, tissue cytoarchitectural alterations seen in a H&E stained 4T1 tumor xenograft sample (i, k) could be complemented with the vascular visibility of the GalRh-BVu polymer in bright field (i, k) and fluorescence microscopy images (j, l). N.B. The brightness and contrast of H&E images were adjusted for visualization purposes without any changes to the original data.

Extended Data Fig. 2 Combining Euclidean distance maps derived from CT with ADC maps derived from DW-MRI in a human breast cancer model.

a-c, A 2D section from the 3D Euclidian distance map (EDM) is shown with an overlay of white contour lines to highlight regions within intervessel distance ranges 0-50 μm (a), 51-150 μm (b) and 151-350 μm (c), respectively. Soft tissue contrast from T1W-MRI data of the same region was employed as the underlay image in (a-c). The contour lines corresponding to the inter-vessel distance ranges shown in (a-c) were mapped on to co-registered apparent diffusion coefficient (ADC) maps derived from DW-MRI (d-f), respectively. Rim and central tumor sub-regions from (d) and (f) were selected and visualized with volume rendered tumor blood vessels (red) derived from CT (g-h). Low ADC regions (blue-green) co-localized with regions with a high density of tumor vasculature (g), while high ADC regions (yellow-red) co-localized with regions exhibiting low vessel density (h). i, Box and whisker plots of whole-tumor ADC distributions showed that 151-350 μm EDM regions were significantly different (p « 0.001) from those for 51-150 μm EDM regions and 0-50 μm EDM regions using a two-tailed Mann-Whitney U-test test at alpha = 0.05. The box and whisker plots corresponding to 0–50 μm, 50-150 μm and 150-350 μm EDM regions show the median, interquartile range (IQR) and the data within the Q1 − 1.5IQR and Q3 + 1.5IQR range. The upper and lower bounds of the displayed intensity range for the merged images shown in (a-f) were adjusted for visualization purposes without any changes to the original data.

Extended Data Fig. 3 Correlation between tumor boundary-to-center profiles for MRI-, CT- and optical imaging-derived vascular microenvironmental (VME) parameters in a human breast cancer model.

a-b, For each VME parameter map (e.g. ADC), we overlaid a 2D grid of points along azimuthal (white points) and radial directions (dashed red lines). An enlarged view of the grid is shown in (b) wherein black arrows point to white contours that are located at the tumor boundary and at 1 mm and 2 mm normal to it. Next, boundary-to-center profiles were calculated along each dashed red line and an average radial profile generated for each VME parameter map. c, ADC correlated with EDM (R2 = 0.43, p = 0.0084). d, Collagen (Col) fractional area correlated inversely with EDM (R2 = 0.35, p = 0.0183). e, FA correlated inversely with ADC (R2 = 0.68, p < 0.0001). f, FA correlated with Col fractional area (R2 = 0.7, p = 0.0001). The Pearson correlation coefficients between each variable pair shown in (a-d) was significant.

Extended Data Fig. 4 Steps for matching sample orientation between CT and MPM imaging.

a, The sample was embedded in an agarose block prior to CT imaging and directional annotations made. Before sectioning the sample for MPM, the location of the cutting plane was determined relative to the tumor center by matching the embedded sample with its T1W-MRI image, as shown in (b). Red hatched line indicate where the sample was cut. This orientation was then preserved with the help of the directional annotations shown in (c) during cutting, and (d) during cryosectioning.

Extended Data Fig. 5 Creating a 4D (that is 3D + time) visualization by mapping the temporal dynamics of the in vivo functional hyperemic response to 3D ex vivo neurovascular and anatomical data.

a, A thinned-skull preparation for in vivo LSC and IOS imaging. b, The animal was made to breathe room air (AIR), carbogen (95% oxygen/5% carbon dioxide) gas (CARB), and room air (AIR) for 3, 2 and 5 minutes, respectively during which dynamic CBF data was acquired. Black arrows in (b) correspond to the time points (that is 0.4 and 2.5 min, AIR; 3.3 and 5 min CARB; and 7.5 and 10 min, AIR) for which the corresponding CBF maps are shown in (f-k). Black, dark gray and light gray squares (d-e) indicate large (i.e. 115 μm < diameter < 120 μm), medium (i.e. 40 μm < diameter < 60 μm) and small (i.e. 20 μm < diameter < 40 μm) blood vessels that were identified using the IOS image (c) and from which the mean in vivo CBF traces shown in (e) computed. e, Medium (dark gray trace) and large vessels (black trace) showed a larger peak increase in %ΔCBF w.r.t the global baseline than that exhibited by small vessels (light gray trace). f-k, Spatio-temporal evolution of CBF corresponding to the experimental paradigm in (b) illustrating the significant response to carbogen inhalation (h, i). l, The same sample prepared for ex vivo imaging in which the GalFITC-BVu perfused neurovasculature was visible (white contrast) in the intact skull. m-o, Concurrent visualization of the 3D skull anatomy (gray) and underlying neurovasculature (red) using ex vivo CT imaging (7.5 μm) (m-o). p, Fluorescent MIP images of perfused skull vessels from a tiled scan acquired at 10× with confocal microscopy (1.3 μm), and a 25× scan of the same sample acquired with MPM (0.6 μm) (q). The positive vascular contrast in CT data (m-o, r-w) was due to BVu while the GalFITC component provided fluorescence contrast in microscopy data (p-q). r-w, Integrated 4D volume created by co-registering the 2D in vivo CBF maps (f-k) to 3D ex vivo neurovascular and skull anatomy data (m-o) illustrating the time evolution of the functional hyperemic response. The displayed intensity range for (f-k) was adjusted for visualization purposes without altering the original data. A 0.25 minute moving average filter was applied to (e) to reduce noise. Scale bars: 1 mm unless stated otherwise.

Extended Data Fig. 6 Validation of the image-based hemodynamic modeling approach.

To validate our blood flow modeling approach, we employed a 546-segment vascular network of the rat mesentery (a) that was derived from high resolution intravital microscopy imaging data by Pries et al15. To simulate pressure and blood flow values in all segments of the network, experimentally obtained blood flow rates were prescribed at 35 boundary segments while one boundary node was subjected to a constant pressure boundary condition. Blood flow and discharge hematocrit distributions in all 546 segments simulated using our approach (black dots) are compared against the solution of the fully determined system as obtained by Pries et al15. We achieved an R2 = 0.99 for blood flow rates (nl/min) and R2 = 0.93 for discharge hematocrit distributions observing excellent agreement between these data. Moreover, the distribution of the ratio of discharge to tube hematocrit vs. vessel diameter satisfied the well-known Fahraeous effect and showed an R2 = 0.94 against the simulated values reported by Pries et al15 (d). Finally, fractional erythrocyte flow (FQE) vs. fractional blood flow (FQB) distributions obtained using our approach satisfied the phase separation effect (e) in agreement with the distributions reported by Pries et al15 (f). Open and filled circles correspond to data points for daughter vessels α and β at diverging bifurcations. Collectively, these plots demonstrate the validity of our image-based hemodynamic modeling approach and its utility for predicting functional properties of micro-vascular networks. Panel (f) reproduced with permission from15.

Extended Data Fig. 7 The GalRh-BVu polymer remained stable for at least 11 months after sample preparation.

a, LSM image of the thalamic vasculature in a murine brain acquired at 0.33 μm spatial resolution at 6 months after sample preparation. b, LSM of the same field of view acquired at 0.56 μm spatial resolution at 11 months after sample preparation. Here, vascular contrast was enhanced by normalizing the image intensity to 0.1% of the dynamic range followed by 3D median filtering (radius = 2 voxels).

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Supplementary Protocols and Tables 1–3.

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Supplementary Video

Video 1. Dynamic functional hyperemic response acquired using in vivo laser speckle imaging (blue-red color map) was integrated to the 3D skull anatomy (gray) and the underlying neurovasculature (red) data acquired ex vivo using CT imaging. The animal was made to breathe room air (AIR), carbogen (95% oxygen/5% carbon dioxide) gas (CARB) and room air (AIR) for 3, 2 and 5 min, respectively, during which dynamic CBF data was acquired. Large (ROI 1) and medium blood vessels (ROI 2) showed a larger peak increase in % ΔCBF with respect to the global baseline than that exhibited by small vessels (ROI 3).

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Bhargava, A., Monteagudo, B., Kushwaha, P. et al. VascuViz: a multimodality and multiscale imaging and visualization pipeline for vascular systems biology. Nat Methods 19, 242–254 (2022). https://doi.org/10.1038/s41592-021-01363-5

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