Association between [⁶⁸Ga]NODAGA-RGDyK uptake and dynamics of angiogenesis in a human cell-based 3D model

Abstract

Radiolabeled RGD peptides targeting expression of α_vβ₃ integrin have been applied to in vivo imaging of angiogenesis. However, there is a need for more information on the quantitative relationships between RGD peptide uptake and the dynamics of angiogenesis. In this study, we sought to measure the binding of [⁶⁸Ga]NODAGA-RGDyK to α_vβ₃ integrin in a human cell-based three-dimensional (3D) in vitro model of angiogenesis, and to compare the level of binding with the amount of angiogenesis. Experiments were conducted using a human cell-based 3D model of angiogenesis consisting of co-culture of human adipose stem cells (hASCs) and of human umbilical vein endothelial cells (HUVECs). Angiogenesis was induced with four concentrations (25%, 50%, 75%, and 100%) of growth factor cocktail resulting in a gradual increase in the density of the tubule network. Cultures were incubated with [⁶⁸Ga]NODAGA-RGDyK for 90 min at 37 °C, and binding of radioactivity was measured by gamma counting and digital autoradiography. The results revealed that tracer binding increased gradually with neovasculature density. In comparison with vessels induced with a growth factor concentration of 25%, the uptake of [⁶⁸Ga]NODAGA-RGDyK was higher at concentrations of 75% and 100%, and correlated with the amount of neovasculature, as determined by visual evaluation of histological staining. Uptake of [⁶⁸Ga]NODAGA-RGDyK closely reflected the amount of angiogenesis in an in vitro 3D model of angiogenesis. These results support further evaluation of RGD-based approaches for targeted imaging of angiogenesis.

Introduction

Integrins are transmembrane glycoprotein receptors that mediate interactions between cells and their surroundings during normal development, and in response to physiological and pathophysiological signals. Integrin α_vβ₃ plays a key role in angiogenesis associated with various disease states, such as ischemic heart disease and during tumor growth [1, 2]. Expression of integrin α_vβ₃ is generally low in endothelial cells but rises during angiogenesis [1], when the receptor also undergoes a conformational change into the active form [3].

Integrin specific ligands containing the tripeptide sequence arginine–glycine–aspartic acid (RGD) have been radiolabeled for non-invasive imaging of integrin expression using single-photon emission computed tomography (SPECT) or positron emission tomography (PET) [4]. Radiolabeled peptides that selectively bind to α_vβ₃ integrin have shown promise for non-invasive imaging of pathological conditions associated with angiogenesis, such as peripheral artery disease, ischemic myocardial injury, stroke and cancer [5–8]. In such studies, the uptake of RGD-based tracers has been associated with histological evidence of angiogenesis. However, some studies have suggested that uptake reflects other processes, such as inflammation [9, 10] and fibrosis [11, 12]. Thus, further evaluation of the relationship between the uptake of RGD-based tracer and dynamics of angiogenesis is needed to understand whether the activity of angiogenesis can be accurately quantified by imaging.

[⁶⁸Ga]NODAGA-RGDyK is a novel ⁶⁸Ga-labeled cyclic 1,4,7-triazacyclononane-1-glutaric acid-4,7-diacetic acid-conjugated RGD peptide designed for PET imaging of α_vβ₃ integrin expression. It has favorable biokinetics, radiation dose, and safety profile [13, 14]. In a previous study using [⁶⁸Ga]NODAGA-RGDyK, we detected an increase in myocardial α_vβ₃ integrin expression in ischemic myocardium, localized within irreversibly injured myocardium, in the absence of an increase in angiogenesis [12]. To further evaluate the ability of [⁶⁸Ga]NODAGA-RGDyK to measure angiogenic activity, we investigated whether binding of this agent reflects the amount of angiogenesis in a human cell-based 3D in vitro model of angiogenesis [15, 16]. This model consisting of a co-culture of human umbilical cord vein endothelial cells (HUVECs) and human adipose stromal cells (hASCs) mimics dynamics of the development of normal human vasculature. After stimulation with growth factors, the cells produce a vascular-like tubule network with morphology of mature vessels within few days. The density of the vascular network can be reproducibly controlled by adjusting concentrations of growth factors.

Materials and methods

Angiogenesis tissue model

We used a human cell-based 3D model of angiogenesis developed at the Finnish Centre for Alternative Methods (FICAM) [15, 16]. When establishing the cell model, hASC cells were thawed, propagated for 9 days, and then seeded onto a plastic coverslip in 24-well plates (for receptor binding studies) or in 2-well chamber microscope slides (for autoradiography studies). On the same day, HUVECs that had been thawed and propagated for 3 days were plated on top of the hASC cell layer to form a co-culture. The next day, stimulation of the vascular-like tubule network formation was initiated by increasing the concentration of vascular endothelial growth factor (VEGF) (R&D Systems, Inc, Minneapolis, US) and fibroblast growth factor β (FGF-β) (R&D Systems, Inc, Minneapolis, US); induction medium was replaced with fresh medium after 3 days. To obtain a gradient in tubule network density, four different growth factor concentrations were used: 10 ng/ml VEGF and 1 ng/ml FGF-β (defined as 100%), and 25%, 50%, and 75% of that maximum concentration. Co-culture of hASCs and HUVECs without induction of a tubule network (because inductive growth factors were not added) served as a control. Cell culture was terminated 6 days after the start of the tubule network stimulation.

Radiochemistry

The tracer precursor, 1,4,7-triazacyclononane-1-glutaric acid-4,7-diacetic acid-conjugated RGD peptide (cyclo[L-arginylglycyl-L-α-aspartyl-D-tyrosyl-N6-([[4,7-bis(carboxymethyl)-1,4,7-triazonan-1-yl]acetyl])-L-lysyl]; NODAGA-RGDyK), was purchased from ABX Advanced Biochemical Compounds GmbH (product number 9805; Radeberg, Germany). ⁶⁸Ga was obtained from a ⁶⁸Ge/⁶⁸Ga generator (Eckert & Ziegler, Valencia, CA, USA) by elution with 0.1 M aqueous hydrochloric acid. ⁶⁸Ga-eluate (500 μl) was mixed with sodium acetate (18 mg) to a pH of approximately 5. NODAGA-RGDyK (10 nmol, dissolved in deionized water to generate a stock solution of 1 mM) was added, and the reaction mixture was heated at 100 °C for 15 min. No further purification was performed. The radiochemical purity of [⁶⁸Ga]NODAGA-RGDyK was determined by reversed-phase high-performance liquid chromatography (HPLC) on a Jupiter C18 column (4.6 × 150 mm, 300 Å, 5 μm; Phenomenex, Torrance, CA, USA). HPLC conditions were as follow: flow rate = 1 ml/min, λ = 220 nm. Gradient system: A = 0.1% trifluoroacetic acid (TFA) in water; B = 0.1% TFA in acetonitrile. A/B gradient: 0–5 min 97/3, and 5–15 min from 97/3 to 0/100. The HPLC system consisted of a LaChrom instrument (Hitachi; Merck, Darmstadt, Germany) coupled with a flow-through radiomatic 150TR radioisotope detector (Packard, Meriden, CT, USA). At the end of the syntheses, radiochemical purity and molar activity of [⁶⁸Ga]NODAGA-RGDyK were ≥ 95% and 11.9 ± 5.9 GBq/µmol, respectively.

In vitro binding of [⁶⁸Ga]NODAGA-RGDyK

Transport medium was removed from the wells, and tissue cultures were incubated in medium for 1 h at 37 °C. The medium was Dulbecco’s modified Eagle’s medium/Nutrient Mixture F-12 (DMEM/F12) supplemented with 2.56 mM L-glutamine, 0.1 nM 3,3’,5-triiodo-L-thyronine sodium salt, 6.65 µg/ml insulin, 6.65 µg/ml transferrin, 6.65 ng/ml selenious acid, 1% bovine serum albumin (BSA), 2.8 mM sodium puryvate, 200 µg/ml ascorbic acid, 0.5 µg/ml heparin, 2 µg/ml hydrocortisone, 10 ng/ml VEGF, and 1 ng/ml FGF-β. Then, the medium was removed, and [⁶⁸Ga]NODAGA-RGD in phosphate-buffered saline (PBS, pH 7.4) was added and incubated for 90 min in 37 °C. Incubation time and temperature were chosen according to a previous study [17]. After the tracer was removed, the cells were washed once with PBS. The cover slips that contained the cells were measured for radioactivity using a gamma counter (Wizard 3″; PerkinElmer/Wallac, Turku, Finland).

In vitro autoradiography

Transport medium was removed from the chamber slides, and warm medium was added. Tissue cultures were incubated for 1 h at 37 °C; medium was removed; and [⁶⁸Ga]NODAGA-RGDyK was added. After incubation for 90 min at 37 °C, the tracer solution was removed, the chamber walls were removed, and the cells were washed twice with PBS. Slides were air dried for 10 min and exposed on a phosphorimaging plate (BAS-TR2025; Fuji Photo Film, Tokyo, Japan) for 1 h. The distribution of radioactivity on the plate was visualized and quantified using a Fluorescent Image Analyzer (Fujifilm FLA-5100, Fuji Photo Film) and the AIDA Image analyzer software v.4.55 (Raytest Isotopenmessgeräte GmbH, Straubenhardt, Germany). Autoradiography uptake was expressed as photostimulated luminescence per square millimeter (PSL/mm²), and the vessel-to-base cell layer ratio was calculated by dividing the uptake of the vessels by the uptake of the base cell layer consisting of hASCs and HUVECs without growth factors.

Immunohistochemistry

After measurements with gamma counter or autoradiography, the tissues were fixed in 70% ethanol for 15 min and stained with antibodies against von Willebrand factor (vWF) and collagen IV. Cells were permeabilized with Triton X-100 for 15 min, and nonspecific binding sites were blocked with 10% BSA for 30 min. Primary antibodies (anti-von Willebrand factor, dilution 1:100; anti-collagen IV, dilution 1:500; Sigma-Aldrich, Saint Louis, Missouri, US) were applied overnight. After washing steps, secondary antibodies (tetramethylrhodamine [TRITC]-conjugated anti-rabbit for von Willebrand factor and fluorescein isothiocyanate [FITC]-conjugated anti-mouse for collagen IV; Sigma-Aldrich, Saint Louis, Missouri, US) were applied for 45 min. Secondary antibodies were washed away, and PBS was left in the wells. Fluorescence imaging of stained tubular structures was performed using a Cell-IQ automated image analysis system (CM-Technologies, Tampere, Finland). The degree of angiogenesis in each image was graded manually; the scoring criterion was the intensity of the vascular-like tubular network (tubule length and branching). The highest score was 5 (dense, highly branched tubular network), and the lowest score was 0 (no or minor tubules). In order to detect α_vβ₃ integrin, tissues were stained with anti-integrin α_vβ₃ antibodies (dilution 1:100, Sigma-Aldrich, Saint Louis, Missouri, US) and Alexa Fluor 488 conjugated anti-mouse secondary antibody.

Statistical analyses

SPSS Statistics software v.25 (IBM, Armonk, NY, USA) was used for statistical analyses. Unpaired Student’s t-test was used for comparisons between two groups, and comparisons between multiple groups were performed using ANOVA with Tukey’s post hoc test. Spearman’s rank test (r_s) was used to analyze correlation. p < 0.05 was considered statistically significant.

Results

In vitro tracer binding

We performed a tracer binding study in a human cell-derived angiogenesis tissue model using four different concentrations of angiogenesis-promoting growth factors, which yielded vascular-like tubule networks of four different densities. The density of tubules gradually increased with growth factor concentration (Fig. 1a). Relative to control cells that were not treated with growth factors, uptake of [⁶⁸Ga]NODAGA-RGDyK was 1.6-fold higher at 25% growth factor concentration, 2.1-fold higher at 50%, 2.4-fold higher at 75%, and 2.5-fold higher at 100%. Relative to the 25% concentration, uptake of [⁶⁸Ga]NODAGA-RGDyK was significantly higher at 75% (p = 0.0003) and 100% (p = 0.0002) (Fig. 1b). [⁶⁸Ga]NODAGA-RGDyK uptake also correlated with the density of vascular-like tubule network, as determined by visual examination of histological staining (Fig. 1c).

Fig. 1.

Representative image of vascular-like tubule networks with different growth factor concentrations of 25%, 50%, 75%, and 100% stained for von Willebrand factor (red) and collagen IV (green) (a). The graph in b shows the vessel-to-base cell layer ratio of [⁶⁸Ga]NODAGA-RGDyK uptake at the indicated growth factor concentrations, and the graph in c shows the correlation between vessel density, and the ratio of [⁶⁸Ga]NODAGA-RGDyK uptake between vessel and base cell layer. Asterisks denote a statistically significant difference relative to a growth factor concentration of 25%. (Color figure online)

Autoradiography

Representative autoradiographs of [⁶⁸Ga]NODAGA-RGDyK uptake in vessels with growth factor concentrations of 75% and 100% are shown in Fig. 2. Uptake was localized in the regions of angiogenesis, indicated by tubule structures positive for vWF and collagen IV, and was significantly higher at 100% vs. 75% growth factor concentration (vessel-to-base cell layer ratio: 3.3 ± 0.09 vs. 2.5 ± 0.63; p = 0.009).

Fig. 2.

Examples of immunohistochemistry and autoradiography at growth factor concentrations of 75% and 100% (a). Tubules were stained for von Willebrand factor (red) and collagen IV (green) in the double-stained images, and for α_vβ₃ integrin (green). Panel b shows [⁶⁸Ga]NODAGA-RGDyK uptake in tissue at growth factor concentrations of 75% and 100%. (Color figure online)

Discussion

In this study, using an in vitro 3D model of angiogenesis, we found that [⁶⁸Ga]NODAGA-RGDyK binding was proportional to the amount of angiogenesis. Our experiments were performed in a human cell-based angiogenesis tissue model consisting of a co-culture of HUVECs and human adipose stromal cells (hASCs), which generate a reproducible, extensive, mature vascular-like tubule network after stimulation with a growth factor cocktail [15, 16]. This is the first study of an RGD targeting tracer in a tissue model that mimics post-infarct angiogenesis. The density of the tubule network increased with the concentration of growth factors. Vessels in this model exhibit mature properties and become surrounded by pericytes [16, 18]. Pericyte coverage is a characteristic of maturation of newly formed vessels in the myocardium after infarction [2], indicating that the model we used accurately represents in vivo angiogenesis. α_vβ₃ integrin also seems to be involved in the maturation process, as evidenced by the fact that anti-α_vβ₃ integrin therapy decreases pericyte coverage in tumor vessels [19]. Our results lend support to the concept that [⁶⁸Ga]NODAGA-RGDyK can be used to quantitatively assess activity of angiogenesis, which is of particular importance for predicting and monitoring therapy responses.

Our results are in line with previous studies showing that the uptake of integrin-targeting RGD peptides is associated with histological evidence of newly formed blood vessels [6], coincides with hypoxia [20], and can be modified by therapy inducing [21, 22] or inhibiting angiogenesis [23]. However, the limited number of time points over prolonged period (for example from 3 days to 3 months after an ischemic insult) does not permit detailed evaluation of association between tracer uptake and ongoing angiogenesis. Furthermore, in addition to mediating angiogenesis, α_vβ₃ integrin also regulates macrophage inflammatory responses and myofibroblast differentiation [24, 25]. Therefore, the uptake of tracers targeting α_vβ₃ integrin may not merely represent angiogenesis, but also other events during the repair process after ischemic myocardial injury. Because multiple cell types express α_vβ₃ integrin, in vivo studies measuring RGD uptake in the context of angiogenesis have yielded conflicting results, as angiogenesis does not always co-localize with integrin expression [9–12]. Studied RGD-based peptides also have different selectivity for different types of integrins [26]. Our in vitro 3D model of angiogenesis provides a more controlled and isolated environment for newly formed vessels that lacks most of the other α_vβ₃ integrin binding cell types, such as myofibroblasts and macrophages, which are present in in vivo models of myocardial ischemia and infarction. This enables specific evaluation of angiogenesis-associated α_vβ₃ integrin expression using α_vβ₃ integrin selective tracer [⁶⁸Ga]NODAGA-RGDyK.

Uptake of [⁶⁸Ga]NODAGA-RGDyK in vessels was elevated in the presence of higher growth factor concentrations and correlated with the abundance of the vessels. Due to problems with tissue attachment on slides at lower concentrations of growth factors, we performed autoradiography analysis only on the slides treated with concentrations of 75% and 100%; this represents a limitation of the study. However, we were able to detect a difference in [⁶⁸Ga]NODAGA-RGDyK binding between the two concentrations measured. Resolution of autoradiography did not allow detailed localization of the tracer signal with individual vessel structures. For this purpose, a different probe including an optical label could be used in experimental setting instead of a [⁶⁸Ga]NODAGA-RGDyK available for clinical use. Finally, detection of angiogenesis with RGD based tracers is dependent on integrin expression. Although α_vβ₃ integrin is typically expressed during angiogenesis, it may not always be present [27] and thus, there may not be tracer uptake under such circumstances.

Conclusions

[⁶⁸Ga]NODAGA-RGDyK correlated with the amount of angiogenesis in a human cell-based in vitro model of angiogenesis indicating that the tracer uptake reflects ongoing angiogenic activity. These results support further evaluation of RGD-based approaches for targeted imaging of angiogenesis in various disease states, such as ischemic heart disease and cancer. However, the possibility of nonspecific binding should be taken into account when performing in vivo imaging studies of angiogenesis.

Author contributions

All authors contributed to the study conception and design. Material preparation, data collection, and analysis were performed by MG, OM, XGL, TT, and OH. All authors contributed to interpretation of data. The first draft of the manuscript was written by MG, and all authors commented on the drafts of the manuscript. All authors read and approved the final manuscript.

Funding

Open access funding provided by University of Turku (UTU) including Turku University Central Hospital. The study was financially supported by the Academy of Finland, the Finnish Foundation for Cardiovascular Research, Sigrid Jusélius Foundation, Maud Kuistila Memorial Foundation, State Research Funding of Turku University Hospital, and Drug Research Doctoral Programme of the University of Turku.

Declarations

Conflict of interest

The authors declare that they have no conflicts of interest pertaining to this work.

Ethical approval

hASCs and HUVECs were isolated from the human fat tissue and umbilical cords, respectively, as permitted by The Regional Ethics Committee of Tampere University Hospital’s Responsibility Area in accordance with the International Conference on Harmonization (ICH) GCP guidelines (CPMP/ICH/135/95), the World Medical Association Declaration of Helsinki (1964), and subsequent amendments.