Adverse drug reactions (ADRs) restrict the maximum doses applicable in chemotherapy, which leads to failure in cancer treatment. Various approaches, including nano-drug and prodrug strategies aimed at reducing ADRs, have been developed, but these strategies have their own pitfalls. A renovated strategy for ADR reduction is urgently needed. Here, we employ an enzymatic supramolecular self-assembly process to accumulate a bioorthogonal decaging reaction trigger inside targeted cancer cells, enabling spatiotemporally controlled, synergistic prodrug activation. The bioorthogonally activated prodrug exhibits significantly enhanced potency against cancer cells compared with normal cells. This prodrug activation strategy further demonstrates high tumour inhibition efficacy with satisfactory biocompatibility, pharmacokinetics, and safety in vivo. We envision that integration of enzymatic and bioorthogonal reactions will serve as a general small-molecule-based strategy for alleviation of ADRs in chemotherapy.
Bitter pills may have wholesome effects. Anticancer drugs, for example, are highly potent but are associated with adverse drug reactions (ADRs), minimization of which is a critical but largely unmet need in cancer treatment1,2. The risk of side effects of these chemo-drugs on normal cell populations and specific organs (e.g. the cardiotoxicity of doxorubicin (Dox)3) limits the applicable dosages. This restricted dosage likely prevents the whole tumour tissue from being exposed to sufficient drug concentrations, eventually resulting in cancer recurrence and metastasis4. A variety of strategies have been implemented to reduce ADRs via either physical5 or chemical control of drug activity, the latter of which is usually referred to as a prodrug, undergoing enzymatic and/or chemical transformations in situ to release the parent drug with desired pharmacological effects6. The development of ideal prodrugs that meet both the following requirements remains challenging: (i) targeted delivery, i.e. the delivery of effective doses of prodrugs directly to the tumour tissue, and (ii) selective activation, i.e. effective activation of prodrugs in tumour-specific environments and virtual inactivity in normal tissues. For example, antibody drug conjugates (ADCs) may often encounter non-specific activation via metabolic hydrolysis of the linker between the antibody and drug7. Antibody-directed enzyme prodrug therapy (ADEPT) introduces exogenous enzymes to improve the orthogonality of drug activation reactions8. However, the introduction of an exogenous enzyme prevents repeated administration due to issues such as immunogenicity9. To address the selective activation issue, the therapeutic potential of the tetrazine (Tz)–trans-cyclooctene (TCO) decaging pair has been recently exploited10. However, one example using this pair as an ADC linker will inevitably be limited by the insufficient penetration ascribed to mAbs11. Another example of the polymeric hydrogel-based application is mainly suitable for local injection to treat resectable tumours because the delivery of toxic agents is highly dependent on the method of gel administration12.
On the other hand, recent progress in in situ enzyme-instructed supramolecular self-assembly (EISA) has demonstrated the enormous potential of this technique in targeted therapeutic applications13,14,15. Starting from small-molecular precursors that undergo enzymatic transformations to initiate the supramolecular self-assembly process, EISA is highly dependent on the activity of specific enzymes16,17. Because the spatiotemporal profile of up- or down-regulated enzymes is quite tumour specific18, EISA could selectively recognize cancer cells by targeting such abnormal enzymatic activities19. For example, by targeting over-expressed phosphatase in HeLa cells, phosphorylated small molecules can be designed that undergo enzymatic dephosphorylation, ultimately leading to the construction of supramolecular assemblies inside live cells20. For cells that have very high phosphatase levels, such as Saos-2 cells, EISA may have direct and strong inhibitory effects via necroptosis21. By systemic administration, these small molecules may diffuse deeply into the tumour and therefore may overcome the disadvantages of insufficient penetration, which is often observed with mAbs22.
Here, we use a combination of EISA and Tz/TCO bioorthogonal decaging reaction which simultaneously leads to spatiotemporal targeting and selective activation of prodrugs inside cancer cells, achieving the urgently needed selectivity of chemo-drugs for cancer cells over normal cells (Fig. 1). We attach a Tz moiety to the EISA motif to directly trigger the inverse-electron-demand Diels–Alder (inv-DA) reaction-mediated chemical decaging of a TCO-caged effector molecule within the intracellular environment23,24,25. Cancer cells over-expressing phosphatase exhibit intracellular EISA via the Tz-bearing NapK(Tz)YF (3). This intracellular EISA results in significant accumulation of Tz inside the cancer cells, enabling the liberation of a TCO-caged prodrug (TCO-Dox) that exerts cytotoxic effects and induces cancer cell death. In contrast, in the absence of EISA, TCO-Dox is hardly activated, and normal cells are left intact. The selectivity of activated Dox for cancer cells over normal cells is enhanced 10–20-fold in comparison with that of native Dox, representing an appealing strategy for ADR reduction. Overall, our strategy enables spatiotemporally controlled, synergistic prodrug activation with superior selectivity for cancer over non-cancer cells, which ultimately leads to effective and safe tumour inhibition, as demonstrated in a xenografted cervical cancer model (HeLa cells) in mice.
Self-assembly and prodrug activation
The synthesis of the assembly precursor (NapK(Tz)YpF, 2, Fig. 2a) was straightforward (see Supplementary Methods for a detailed protocol). Because KYF was determined to be an excellent self-assembly motif in a tri-peptide census survey26, we constructed our assembling molecules based on this sequence. The conjugation of a strong π–π stacking moiety, namely, a naphthalene group, to the N terminus may further enhance the self-assembly potential of this molecule. Phosphorylation on tyrosine (Y) enabled the responsiveness of this motif to phosphatase. All of these components were sequentially conjugated via typical Fmoc-based solid-phase peptide synthesis (SPPS) to yield NapKYpF (1). The capability of self-assembly and hydrogelation of 1 was confirmed by the addition of 10 U mL−1 alkaline phosphatase (ALP) into a solution of 1 (Supplementary Fig. 1). The dephosphorylated product of 1 formed transparent hydrogels with a network of uniform nanofibres (Supplementary Fig. 2), and the critical hydrogelation concentration was 1.0 mg mL−1. The ε-amine of Lys on 1 was conjugated with the Tz derivative Tz-COOH (2-(4-(6-methyl-1,2,4,5-tetrazin-3-yl)phenyl) acetic acid) via an NHS-mediated ester–amide exchange reaction to yield 2. Aryl-substituted Tzs are commonly used in inv-DA reactions, and a methyl group could significantly promote the decaging rate. Upon the addition of ALP (10 U mL−1) into the solution of 2, a transparent purple hydrogel was formed within 1 h (Fig. 2b inset), and the critical hydrogelation concentration was 1.0 mg mL−1 (Supplementary Fig. 3). Similar to the formation of a typical hydrogel, investigation by transmission electron microscopy (TEM) confirmed the existence of numerous uniform nanofibres, each with a diameter of approximately 12 nm, which was close to that of hydrogel 1 (Fig. 2b). A further oscillatory rheological test also confirmed the formation of a stable hydrogel of 2, as demonstrated by the following observations: (i) the dynamic storage modulus (G′) of the hydrogel was almost one order of magnitude higher than the dynamic loss modulus (G″), and (ii) the frequency dependence of the elasticity was weak (Fig. 2c and Supplementary Fig. 4).
The Tz counterpart prodrug TCO-Dox was prepared according to previously published procedures using the axial tautomer of TCO27. After the selection of optimized Tz and TCO, the decaging reactions in our study were further characterized (Fig. 2d). After mixing 2 μL of 10 mM TCO-Dox with 2.5 μL of 20 mM 2 in 25% acetonitrile in H2O at 37 °C, the reaction mixture was analysed by ultra-performance liquid chromatography-mass spectrometry (UPLC-MS) at different time points. As shown in Fig. 2e, with 2, TCO-Dox and Dox as references, the LC trace clearly showed the disappearance of the TCO-Dox peak 2 min after TCO-Dox was mixed with 2. The emerging peak a, representing Dox, remained unchanged between 2 and 30 min, which indicated complete liberation of Dox within 2 min. The TCO adduct (peak b) exhibited a similar retention time as 2 (peak c), and these two neighbouring peaks were further identified by mass spectroscopy (Supplementary Fig. 5). Similarly, we prepared TCO-caged coumarin (TCO-CMR, see Supplementary Methods for a detailed synthesis protocol)23. According to a previously developed fluorescence liberation27, the fluorescence of coumarin was restored rapidly in the presence of Tz derivatives (Supplementary Fig. 6). Notably, the morphology of the nanofibres remained unchanged with the TCO adduct after liberation of Dox (Supplementary Fig. 7). Overall, we showed that the conjugation of Tz with the assembled molecules retained the decaging capability of Tz against TCO derivatives with high reactivity and liberation rates.
Occurrence and localization of self-assembly in live cells
Next, we tested the intracellular accumulation of Tz via EISA in an attempt to differentiate cancer cells from normal cells28. First, we investigated the accumulation of Tz in HeLa cells and HUVECs over time via fluorescence liberation from TCO-CMR (Fig. 3a). Each group of cells was pre-incubated with different concentrations of 2 ranging from 100 to 500 μM for 1, 2, 4, 6, 15 or 24 h. The cells were then washed with PBS thoroughly before the addition of an excessive amount of TCO-CMR (100 μL, 50 μM), and the reaction of TCO-CMR with the intracellular accumulated Tz was allowed to proceed for up to 24 h (Supplementary Fig. 8). In this experimental setting, the total liberated fluorescence was proportional to the amount of 3 accumulated inside the cells. As shown in Fig. 3b, a very small amount of fluorescence was restored in HeLa cells incubated with 100–300 μM 2, and similar results were observed when HeLa cells were incubated with 50 or 500 μM Tz-COOH for 24 h (Supplementary Fig. 9). In contrast, the fluorescence emission increased significantly in HeLa cells pre-incubated with 400 or 500 μM 2. Notably, when incubated with 500 μM 2, the fluorescence in HeLa cells increased proportionately to the incubation time until reaching a maximum value at approximately 6 h. These observations suggested that (i) 500 μM 2 was sufficient for intracellular accumulation of Tz and (ii) six hours of incubation was adequate for the accumulation to reach a saturated state. In contrast to HeLa cells, HUVECs liberated only a negligible amount of fluorescence, even in the presence of 500 μM 2, implying that EISA barely occurred in the normal cells (Supplementary Fig. 10). Therefore, the optimized concentration of 2 (e.g. 500 μM) and incubation time (e.g. 6 h) were selected to differentiate between cancer and normal cells according to liberated fluorescence intensity (Fig. 3c). This differentiation was dependent on the considerably different phosphatase activity between these cell lines (Supplementary Fig. 11), allowing EISA to specifically occur in cancer cells as opposed to normal cells. Further incubation of HeLa cells with the phosphatase inhibitor led to a significant decrease in liberated coumarin (Supplementary Fig. 12), indicating that the accumulation of Tz in HeLa cells was positively correlated with the upregulated phosphatase activity.
In addition to the accumulation profile, we monitored the location of EISA inside cells. First, HeLa cells were incubated with 500 μM 2 for 6 h before being subjected to fractionation29. TEM images of the cellular fractions M (mitochondria, lysosomes, peroxisomes) and P (plasma membrane, microsomal fraction (fragments of the endoplasmic reticulum (ER)), large polyribosomes) of the treated cells showed the presence of nanofibres (Supplementary Fig. 13), verifying the occurrence of nanofibre formation inside HeLa cells. Furthermore, we used confocal fluorescence microscopy to visualize the location of EISA. HeLa cells pre-incubated with 500 μM 2 for 6 h were thoroughly washed with PBS to remove any remaining diffusive 2 or 3. Before the addition of TCO-CMR to the cells (0 min in Fig. 3d), no blue fluorescence of coumarin was detected. Interestingly, a bright fluorescent area appeared near the nucleus within 30 s after the addition of TCO-CMR, indicating the high reactivity of the accumulated Tz anchored on intracellular assemblies (Fig. 3d and Supplementary Fig. 14). Time-course imaging showed that the fluorescence of coumarin continued to increase within the first 15 min (Supplementary Movies 1-2), indicating the abundance of Tz inside the cells. The blue fluorescence was near the nucleus, indicating the location of EISA inside HeLa cells (Supplementary Movie 3). Because this observation was relevant to our previous results20, co-staining with an ER tracker (Glibenclamide BODIPY® TR, red channel) further confirmed that EISA occurred on the ER (Fig. 3d). Notably, no additional washing was required after the addition of TCO-CMR during the entire imaging process because of the low fluorescence emission from TCO-CMR. This clean background was critical for real-time visualization of fluorescence enhancement in live cells. Parallel incubation and imaging experiments were conducted with HUVECs, and only weak fluorescence was observed (Supplementary Fig. 15 and Supplementary Movie 4). This result was also consistent with previous fluorescence intensity measurements (Supplementary Fig. 10).
Prodrug activation in live cells
Before studying prodrug activation in EISA pre-targeted cells, we verified the biocompatibility of 2 by measuring the viability of HeLa cells and HUVECs incubated with 2. Based on a standard MTT assay, the viability of both HeLa cells and HUVECs remained >85% after incubation with 500 μM 2 for 24 h (Supplementary Fig. 16). Based on a clonogenic assay30, the surviving fractions of both HeLa cells and HUVECs were more than 75% after treatment with 500 μM 2 for 6 h (Supplementary Fig. 17 and Supplementary Table 1). These results proved that 2 was biocompatible and that the corresponding intracellular assemblies were eligible for further prodrug activation in live cells.
After demonstrating the biocompatibility and targeting capability of EISA, we next explored the anticancer efficacy of EISA via activation of TCO-Dox inside live cells. As a potential prodrug, we expected TCO-Dox to be less toxic than Dox until activation inside targeted cancer cells. We first investigated the cytotoxicity of Dox and TCO-Dox against HeLa cells and HUVECs. As shown in Fig. 4a, b and Table 1, TCO-Dox was much less effective at inhibiting the growth of HeLa cells than native Dox, exhibiting an EC50 value of 6.793 μM, which was nearly 10-fold higher than that of Dox (0.732 μM). Similarly, the EC50 of TCO-Dox against HUVECs was 5.808 μM, which was more than 40-fold higher than that of Dox (0.133 μM). The increased EC50 value validated the reduced potency of TCO-Dox. Nonetheless, TCO-Dox and Dox exhibited no selectivity for HeLa cells and HUVECs, while the EC50 values of both were higher against HeLa cells than against HUVECs.
The use of EISA enhanced the anticancer capability by reversing the potency of TCO-Dox against HeLa cells and HUVECs. Based on the optimized conditions obtained in the aforementioned TCO-CMR activation assay, HeLa cells were pre-incubated with 500 μM 2 for 6 h, thoroughly washed with PBS, and then incubated with TCO-Dox for 72 h. The EC50 of activated Dox against HeLa cells was as low as 0.0298 μM, representing a 228-fold increase in cytotoxicity compared with that of the TCO-Dox prodrug alone (6.793 μM). This dramatically enhanced cytotoxicity indicated that TCO-Dox was effectively activated in HeLa cells. Moreover, the cytotoxicity of this activated Dox was approximately 25 times higher than that of native Dox (EC50, 0.732 μM), which was likely due to the high local concentration of activated Dox in cancer cells than the administration of the native drug itself31. Because the 2/3 levels in HUVECs were negligible, the EC50 of activated Dox was 0.272 μM against HUVECs pre-treated with 500 μM 2, which was approximately 9-fold higher than that against HeLa cells (0.0298 μM). To better illustrate the advantages of EISA-activated Dox, we calculated the ratio of the EC50 value against HUVECs to that against HeLa cells (Table 2). The ratios for TCO-Dox, native Dox and EISA-activated Dox were 0.855, 0.182 and 9.128, respectively, which demonstrated the improved safety (~50-fold enhancement) of our chemically activated Dox over native Dox.
The generality of this prodrug activation strategy was further validated in additional cell lines, including Saos-2 and CCC-HEH-2 cells. Saos-2 is an osteosarcoma cell line that with extremely high expression levels of phosphatase32, while CCC-HEH-2 is a cardiomyocyte primary cell line obtained from human embryonic myocardial tissue. Clinical data has shown severe cardiotoxicity to be induced by Dox3,33, which is consistent with the lower EC50 against CCC-HEH-2 cells (at 0.084 μM) than against HeLa or Saos-2 cells (Fig. 4c, d and Table 1). However, upon treatment with 2 and TCO-Dox as described previously, the EC50 of activated Dox was 0.404 μM against CCC-HEH-2 cells, which confirmed the satisfactory tolerance. In contrast, the EC50 of activated Dox was approximately 0.1 nM against Saos-2 cells. Notably, this low EC50 value was contributed to not only activated Dox but also the emerging toxicity of EISA itself21. As the MTT assay with Saos-2 cells showed relatively low starting levels (Fig. 4c), we further tested the cytotoxicity of 2 against Saos-2 cells by both the MTT assay and clonogenic assay (Supplementary Figs. 16 and 17 and Supplementary Table 1). The results indicated that while the assemblies were compatible with the other cell lines that we tested, they were toxic to Saos-2 cells to some extent, which was likely due to the extremely high phosphatase activity in this cell type (Supplementary Fig. 11). Overall, EISA-activated Dox exhibited high toxicity against cancer cells but not against normal cells (Table 2).
In addition, we demonstrated that EISA formation was essential for the enhanced cytotoxicity of TCO-Dox observed in cancer cells. Similar to the above drug efficacy test, HeLa cells and HUVECs were pre-incubated with 2 at a concentration of 300 μM for 6 h (EISA was hardly observed inside cells under these conditions, Fig. 3c) before the addition of TCO-Dox for measurement of EC50 values. As shown in Supplementary Fig. 18, the EC50 against HeLa cells was 1.199 μM, which was approximately 40-fold higher than that of group incubated with 500 μM 2 (EC50 = 0.0298 μM). Consistent with the coumarin liberation results, the sharp increase in the EC50 value was most likely due to the relatively low accumulation of Tz in HeLa cells. For HUVECs, the EC50 value against TCO-Dox varied little (0.367 μM to 0.272 μM) when the concentration of 2 increased from 300 μM to 500 μM, indicating the wide selectivity window of our EISA for cancer cells over normal cells.
In vivo anticancer efficacy
To evaluate the tumour specificity and in vivo distribution of 2, a mixture of 50 mg kg−1 2 and 0.875 mg kg−1 125I-labelled 2 was intravenously (i.v.) injected into BALB/c nude mice bearing subcutaneous HeLa tumours, which were followed by single-photon emission computed tomography/computed tomography (SPECT/CT) imaging. Figure 5a shows the distribution of 2/3 at different time points. Within the first hour, 2/3 was mainly accumulated in the tumour and liver. Then, 2/3 was gradually cleared and almost removed from the mouse body within 24 h, guaranteeing the safety of this assembly. In the control group injected with 0.875 mg kg−1 125I-labelled 2 alone, almost no 2/3 was accumulated in the tumour site (Fig. 5b), indicating that EISA did not occur in the tumour in the absence of sufficient assembly precursors.
Next, we applied UPLC-MS/MS to examine the pharmacokinetics34 of i.v. administered 2 and the corresponding dephosphorylated 3 in blood, liver and tumour samples from tumour-bearing mice (Fig. 5c). Due to the presence of phosphatases in blood, 2 was partially transformed to the dephosphorylated product 3 in plasma (Supplementary Fig. 19). However, in contrast to the rapid clearance of 2/3 from blood (nearly complete 2 h post injection), the total concentrations of 2/3 in tumours were maintained at high levels for the first 2 h. In particular, the concentration of 3 in tumours increased significantly within 1 h, indicating specific accumulation in tumours over liver or blood, which is attributed to the phosphatase upregulation of HeLa cells. To avoid unwanted activation of the TCO-Dox prodrug in blood, we chose a 2-h interval between the administration of 2 and TCO-Dox. As shown in Fig. 5d, TCO-Dox was effectively activated in tumours to provide a high and sustained concentration of Dox (at least 24 h after injection of TCO-Dox), which was dependent on tumour-specific accumulation of 2/3 and relatively high concentration of TCO-Dox remaining in the blood (Supplementary Fig. 20). In comparison, the concentration of activated Dox remained very low in the liver, and it was almost undetectable in the blood within 24 h (Fig. 5d). For example, the concentration of activated Dox in tumours was >10-fold higher than that in liver or blood 4 h after TCO-Dox administration, indicating the high tumour specificity of our EISA-enabled prodrug activation strategy.
Finally, to investigate the antitumour efficacy in vivo, HeLa tumour-bearing BALB/c nude mice were randomly allocated into five groups (n = 8) when the tumour volume reached 80–100 mm3. The treatment group received a dose of 50 mg kg−1 2 and a dose of 30 mg kg−1 TCO-Dox after 2-h intervals (abbreviated as 2-2 h-TCO-Dox). Variations in the dose of 2 or TCO-Dox or the interval may slightly curtail the overall tumour inhibition efficacy (Supplementary Fig. 21). For comparison, the remaining four control groups received 50 mg kg−1 2, 30 mg kg−1 TCO-Dox, 5 mg kg−1 Dox or saline. After three courses of treatment, tumour growth was markedly inhibited in the 2-2 h-TCO-Dox treatment group (Fig. 5e). The tumour volume in the saline control group increased rapidly. The tumours treated with 50 mg kg−1 2 or 30 mg kg−1 TCO-Dox alone exhibited rapid growth similar to that observed in the saline control group. For the group that received native Dox, although tumour growth could be inhibited with 5 mg kg−1 Dox, the body weight decreased substantially (Fig. 5f). Further increase in the Dox dose resulted in mouse death (Supplementary Fig. 22), indicating the systemic toxicity of Dox in mice. In contrast, the body weights of mice in the 2-2 h-TCO-Dox group remained steady after treatment, indicating the satisfactory biosafety of our strategy.
After treatment for 14 days, the mice were sacrificed, and tumours were dissected (Fig. 5g) for histological examination with haematoxylin–eosin (HE) staining. As shown in Fig. 5h, the 2-2 h-TCO-Dox treatment group exhibited necrotic lesions of the tumours, exhibiting cell shrinkage, loss of contact and coagulation, which was similar to the tumours treated with Dox. These observations indicated that tumour cells can be efficiently destroyed by activated Dox. However, histopathological images of the tumours treated with saline, 2 or TCO-Dox demonstrated that the HeLa cells remained normal. To further assess possible systemic toxicity, the major organs were harvested for histological analysis. The 2-2 h-TCO-Dox treatment group did not exhibit any observable differences compared to the saline control group based on histological examination of the heart, liver, spleen, lung and kidney (Supplementary Fig. 23), further indicating the good biocompatibility and safety of our prodrug strategy.
We have developed a small-molecule-based strategy for anticancer drug delivery with the advantage of ADR alleviation. The concept of integrating enzymatic reaction-triggered supramolecular self-assembly and bioorthogonal cleavage reaction-triggered chemical decaging enabled spatiotemporally controlled prodrug activation. Specifically, by targeting cancer cells over-expressing phosphatase, including HeLa and Saos-2 cells, Tz-bearing assembly precursors were efficiently dephosphorylated and self-assembled due to increased hydrophobicity. The formation of these assemblies significantly increased the local concentration of the assembly molecules with high levels of accumulation of Tz moieties. This bioorthogonally reactive handle was able to react with TCO and release the caged cargo. As shown in this study, intracellular self-assembly led to high levels of accumulation of Tz in cancer cells, which guaranteed rapid and specific activation of TCO-Dox and facilitated target engagement of the activated Dox inside the nucleus. The overall results showed not only a great increase in the potency of Dox against malignant cells but also the satisfactory selectivity for cancer over non-cancer cells, which indicated the synergistic effects of these two approaches in the alleviation of ADRs. Animal studies further validated not only the biosafety of our EISA compounds and TCO-Dox prodrug but also the excellent in vivo tumour inhibition within a clinically relevant setting. Notably, the dose applied in the current study was below the maximum tolerant dose (MTD) of Dox. Therefore, maximal therapeutic effect may be achieved with a higher dose of TCO-Dox by increasing the number of injections. Given that the TCO-caging method is compatible with various functional groups35, our strategy presented here could be applied to other cytotoxic drugs or toxins that are currently unsuitable for medical use, which may significantly expand the scope of anticancer therapeutic agents. Finally, the subcellular location of the EISA-triggered accumulation of the assemblies (e.g. near microtubules) could be leveraged to bring certain toxins (e.g. maytansine) in close proximity to the corresponding cellular targets with further enhancement of therapeutic effects.
EISA in live cells
All cells were purchased from the National Infrastructure of Cell Line Resource (Beijing, China). HeLa cells, HUVECs and CCC-HEH-2 cells were cultured in a humidified CO2 (5%) incubator at 37 °C in DMEM supplemented with 10% foetal bovine serum (FBS, Gibco) and 1% Pen Strep (PS, Gibco). Saos-2 cells were cultured in a humidified CO2 (5%) incubator at 37 °C in McCoy’s 5A medium supplemented with 10% FBS and 1% PS. Cells were plated in flat-bottom 96-well plates (Corning) at a density of 104 cells per well and allowed to attach for 12 h. Then, the culture medium was replaced with 100 μL of pre-warmed medium containing 2 at different concentrations (100–500 μM). After incubation for different durations (1–24 h), the cells were rinsed with PBS, and then 100 μL of 50 μM TCO-CMR (dissolved in PBS) was added for real-time detection of the fluorescence intensity of coumarin in a plate reader (Perkin Elmer).
Live cell imaging
Cells were first placed in a glass chamber and cultured with 2 mL of culture medium containing 500 μM 2 for 6 h. Then, the cells were rinsed with PBS and incubated with pre-warmed staining solution (500 nM ER-Tracker™ Red dye) for 30 min at 37 °C. The cells were rinsed again with PBS at least five times. After the cell-containing glass chamber was fixed on the confocal microscope stage, 1 mL of 50 μM TCO-CMR (dissolved in PBS) was added, and fluorescent images/movies were captured immediately.
Cells were plated in flat-bottom 96-well plates at a density of 3 × 103 cells per well. After 12 h of cell attachment, the cell culture medium was replaced with 100 μL of pre-warmed media containing the compounds at different concentrations. After 24–72 h of incubation, cell proliferation was assessed by the MTT assay. A fresh mixture of 10 μL of thiazolyl blue tetrazolium bromide (MTT) and 90 μL of medium were freshly added to each well. After incubation for 4 h, the medium was gently removed. The formazan crystals that formed were dissolved in 110 μL of DMSO, and the absorbance was subsequently measured with a plate reader (Perkin Elmer) at 490 nm. EC50 values were calculated using Origin software. To measure the cytotoxicity of 2, HeLa cells, HUVECs, Saos-2 cells and CCC-HEH-2 cells were incubated with 100 μL of 1–500 μM 2 for 24 h, and then, cell viability was determined. To measure the cytotoxicity of TCO-Dox or Dox, HeLa cells, HUVECs, Saos-2 cells or CCC-HEH-2 cells were incubated with 200 μL of 0.001–10 μM TCO-Dox or Dox for 72 h, and the cell viability was determined. To determine the cytotoxicity of activated Dox, HeLa cells, HUVECs, Saos-2 cells or CCC-HEH-2 cells were pre-incubated with 100 μL of 500 μM 2 for 6 h, and then, 2 was removed and 200 μL of 0.0001–10 μM TCO-Dox was added for 72 h of incubation, and cell viability was determined.
All animal studies were performed in accordance with the Institutional Animal Use and Care Regulations approved by the National Institutes of Health Clinical Center/Animal Care and Use Committee (NIH CC/ACUC). Athymic female nude mice (5–6 weeks old) were purchased from Beijing Huafukang Bioscience Co., Ltd., and raised in a specific-pathogen-free barrier facility. Tumour-bearing mice were established by subcutaneously injecting a suspension of 106 HeLa cells per mouse into the front flank of each nude mouse.
The tumour-bearing mice were used for SPECT/CT imaging once the tumour volume reached approximately 200 mm3. For the preparation of 125I-labelled 2, 60 μg of 2 was dissolved in 150 μL of phosphate buffer (pH = 7.0) in a vial coated with 20 μg of iodogen (Sigma, St. Louis, MO). Then, 9 μL of Na125I (2.4 mCi) (Beijing Atom High Tech, Beijing, China) was added, and the mixture was kept at room temperature for 1 h until the labelling ratio reached more than 95%. For SPECT/CT imaging, a mixture of 50 mg kg−1 2 and 0.875 mg kg−1 125I-labelled 2 (700 μCi) was i.v. administered to investigate the distribution of 2/3, and 0.875 mg kg−1 125I-labelled 2 (700 μCi) was administered as a control. After anaesthetization with 2% isoflurane in oxygen, SPECT and helical CT scans of the mice were performed at 2, 5, 7 and 25 h on a NanoScan SPECT/CT imaging system (Mediso, Budapest, Hungary).
When the tumour volume reached approximately 200 mm3, five mice in each group were used for pharmacokinetic analyses of compound 2/3 and for in vivo prodrug activation. For the pharmacokinetic study of compound 2/3, mice received an i.v. injection of 50 mg kg−1 2. For in vivo prodrug activation, mice received an i.v. injection of 50 mg kg−1 2 and a subsequent 30 mg kg−1 TCO-Dox after a 2-h interval. After different time intervals, blood samples were collected from the tail veins, and then, the tumours and livers were harvested for UPLC-MS/MS analysis.
Tumour inhibition test
When the tumour volume reached approximately 80–100 mm3, the mice were divided into five groups (n = 8) and used for therapeutic studies. Mice in the treatment group received an i.v. injection of 50 mg kg−1 2 and a subsequent 30 mg kg−1 TCO-Dox after a 2-h interval. In the control groups, mice were received 50 mg kg−1 2, 30 mg kg−1 TCO-Dox, 5 mg kg−1 Dox or saline. The mice received three treatment courses on day 0, day 3 and day 6. Tumour size and body weight were measured every 2 days. After 14 days, the mice were sacrificed. Tumours and main organs were obtained for histological examination with HE staining.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
A reporting summary for this article is available as a Supplementary Information file. Data that support the findings reported herein are available on reasonable request from the corresponding author.
Miller, M. A. et al. Nano-palladium is a cellular catalyst for in vivo chemistry. Nat. Commun. 8, 15906 (2017).
Rossin, R. et al. Chemically triggered drug release from an antibody–drug conjugate leads to potent antitumour activity in mice. Nat. Commun. 9, 1484 (2018).
Zhang, S. et al. Identification of the molecular basis of doxorubicin-induced cardiotoxicity. Nat. Med. 18, 1639–1642 (2012).
Dubowchik, G. M. & Walker, M. A. Receptor-mediated and enzyme-dependent targeting of cytotoxic anticancer drugs. Pharmacol. Ther. 83, 67–123 (1999).
Barenholz, Y. Doxil—the first FDA-approved nano-drug: lessons learned. J. Control. Release 160, 117–134 (2012).
Huttunen, K. M., Raunio, H. & Rautio, J. Prodrugs—from serendipity to rational design. Pharmacol. Rev. 63, 750–771 (2011).
Wu, A. M. & Senter, P. D. Arming antibodies: prospects and challenges for immunoconjugates. Nat. Biotechnol. 23, 1137–1146 (2005).
Kerr, D. E., Li, Z. G., Siemers, N. O., Senter, P. D. & Vrudhula, V. M. Development and activities of a new melphalan prodrug designed for tumor-selective activation. Bioconjug. Chem. 9, 255–259 (1998).
Sharma, S. K. & Bagshawe, K. D. Antibody directed enzyme prodrug therapy (ADEPT): trials and tribulations. Adv. Drug Deliv. Rev. 118, 2–7 (2017).
Rossin, R. et al. Triggered drug release from an antibody–drug conjugate using fast “click-to-release” chemistry in mice. Bioconjug. Chem. 27, 1697–1706 (2016).
Dreher, M. R. et al. Tumor vascular permeability, accumulation, and penetration of macromolecular drug carriers. J. Natl Cancer Inst. 98, 335–344 (2006).
Oneto, J. M. M., Khan, I., Seebald, L. & Royzen, M. In vivo bioorthogonal chemistry enables local hydrogel and systemic pro-drug to treat soft tissue sarcoma. ACS Cent. Sci. 2, 476–482 (2016).
Ye, D. J. et al. Bioorthogonal cyclization-mediated in situ self-assembly of small-molecule probes for imaging caspase activity in vivo. Nat. Chem. 6, 519–526 (2014).
Zhou, J., Du, X. W. & Xu, B. Regulating the rate of molecular self-assembly for targeting cancer cells. Angew. Chem. Int. Ed. 55, 5770–5775 (2016).
Yang, C. H. et al. Dual fluorescent- and isotopic-labelled self-assembling vancomycin for in vivo imaging of bacterial infections. Angew. Chem. Int. Ed. 56, 2356–2360 (2017).
Li, L. L. et al. Pathological-condition-driven construction of supramolecular nanoassemblies for bacterial infection detection. Adv. Mater. 28, 254–262 (2016).
Pires, R. A. et al. Controlling cancer cell fate using localized biocatalytic self-assembly of an aromatic carbohydrate amphiphile. J. Am. Chem. Soc. 137, 576–579 (2015).
Uhlen, M. et al. Tissue-based map of the human proteome. Science 347, 6220 (2015).
Feng, Z. Q. Q., Wang, H. M., Zhou, R., Li, J. & Xu, B. Enzyme-instructed assembly and disassembly processes for targeting downregulation in cancer cells. J. Am. Chem. Soc. 139, 3950–3953 (2017).
Gao, Y., Shi, J. F., Yuan, D. & Xu, B. Imaging enzyme-triggered self-assembly of small molecules inside live cells. Nat. Commun. 3, 1033 (2012).
Zhou, J., Du, X. W., Yamagata, N. & Xu, B. Enzyme-instructed self-assembly of small D-peptides as a multiple-step process for selectively killing cancer cells. J. Am. Chem. Soc. 138, 3813–3823 (2016).
Huang, P. et al. Tumor-specific formation of enzyme-instructed supramolecular self-assemblies as cancer theranostics. ACS Nano 9, 9517–9527 (2015).
Li, J., Jia, S. & Chen, P. R. Diels–Alder reaction-triggered bioorthogonal protein decaging in living cells. Nat. Chem. Biol. 10, 1003–1005 (2014).
Versteegen, R. M., Rossin, R., ten Hoeve, W., Janssen, H. M. & Robillard, M. S. Click to release: instantaneous doxorubicin elimination upon tetrazine ligation. Angew. Chem. Int. Ed. 52, 14112–14116 (2013).
Wang, J. & Chen, P. R. Development and applications of bioorthogonal cleavage reactions. Acta Chim. Sin. 75, 1173–1182 (2017).
Frederix, P. W. J. M. et al. Exploring the sequence space for (tri-) peptide self-assembly to design and discover. Nat. Chem. 7, 30–37 (2015).
Fan, X. Y. et al. Optimized tetrazine derivatives for rapid bioorthogonal decaging in living cells. Angew. Chem. Int. Ed. 55, 14046–14050 (2016).
Gao, Y. et al. Probing nanoscale self-assembly of nonfluorescent small molecules inside live mammalian cells. ACS Nano 7, 9055–9063 (2013).
Dopp, E. et al. Subcellular distribution of inorganic and methylated arsenic compounds in human urothelial cells and human hepatocytes. Drug Metab. Dispos. 36, 971–979 (2008).
Franken, N. A. P., Rodermond, H. M., Stap, J., Haveman, J. & van Bree, C. Clonogenic assay of cells in vitro. Nat. Protoc. 1, 2315–2319 (2006).
Svensson, H. P. et al. In-vitro and in-vivo activities of a doxorubicin prodrug in combination with monoclonal-antibody beta-lactamase conjugates. Cancer Res. 55, 2357–2365 (1995).
Zhou, J. et al. Enzyme-instructed self-assembly for spatiotemporal profiling of the activities of alkaline phosphatases on live cells. Chem 1, 246–263 (2016).
Petersen, G. H., Alzghari, S. K., Chee, W., Sankari, S. S. & La-Beck, N. M. Meta-analysis of clinical and preclinical studies comparing the anticancer efficacy of liposomal versus conventional non-liposomal doxorubicin. J. Control. Release 232, 255–264 (2016).
Ursuegui, S., Recher, M., Krezel, W. & Wagner, A. An in vivo strategy to counteract post-administration anticoagulant activity of azido-Warfarin. Nat. Commun. 8, 15242 (2017).
Versteegen, R. M. et al. Click-to-Release from trans-cyclooctenes: mechanistic insights and expansion of scope from established carbamate to remarkable ether cleavage. Angew. Chem. Int. Ed. 57, 10494–10499 (2018).
This work was supported by National Key R&D Program of China (2017YFA0205901 to Y.G. and 2016YFA0501501 to P.R.C.), NSFC (21675036 to Y.G. and 21521003 to P.R.C.) and Hundred Talents Project of the Chinese Academy of Sciences for financial support. We also thank F.F. He (National Center for Nanoscience and Technology) for developing the UPLC-MS/MS analysis methods.
The authors declare no competing interests.
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Yao, Q., Lin, F., Fan, X. et al. Synergistic enzymatic and bioorthogonal reactions for selective prodrug activation in living systems. Nat Commun 9, 5032 (2018). https://doi.org/10.1038/s41467-018-07490-6
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