Fluorescent Arylphosphonic Acids: Synergic Interactions between Bone and the Fluorescent Core.

Herein, we report the third generation of fluorescent probes (arylphosphonic acids) to target calcifications, particularly hydroxyapatite (HAP). In this study, we use highly conjugated porphyrin-based arylphosphonic acids and their diesters, namely 5,10,15,20-tetrakis[m-(diethoxyphosphoryl)phenyl]porphyrin (m-H8 TPPA-OEt8 ) and 5,10,15,20-tetrakis [m-phenylphosphonic acid]porphyrin (m-H8 TPPA), in comparison with their positional isomers 5,10,15,20-tetrakis[p-(diisopropoxyphosphoryl)phenyl]porphyrin (p-H8 TPPA-iPr8 ) and 5,10,15,20-tetrakis [p-phenylphosphonic acid]porphyrin (p-H8 TPPA), which have phosphonic acid units bonded to sp2 carbon atoms of the fluorescent core. The conjugation of the fluorescent core is thus extended to the (HAP) through sp2 -bonded -PO3 H2 units, which generates increased fluorescence upon HAP binding. The resulting fluorescent probes are highly sensitive towards the HAP in rat bone sections. The designed probes are readily taken up by cells. Due to the lower reported toxicity of (p-H8 TPPA), these probes could find applications in monitoring bone resorption or adsorption, or imaging vascular or soft tissue calcifications for breast cancer diagnosis etc.

Dysregulation of calcium and phosphate homeostasis often leads to the pathological deposition of minerals, such as calcium <span class="Chemical">carbonate (CC), calcium oxalate (CO), calcium phosphate (CP), calcium pyrophosphate (CPP), and <span class="Chemical">hydroxyapatite (HAP) in many soft tissues,1, 2 such as those in the brain,3 eye,4 kidney5 and skin.2, 6 The pathological deposition of these minerals causes these tissues to become inflexible or even brittle, which can lead to uncontrolled access of extracellular materials or prevent the passive diffusion of molecules between cells and their environment, likely leading to cell death.6 In addition, minerals like HAP can facilitate the retention of molecules by providing a binding surface for the pathological accumulation of molecules.7a Detecting and monitoring increased calcification can be a valuable early indication of breast cancer.8 Conversely, monitoring the decrease in mineralization can be useful for assessing osteoporosis.9 In addition, evidence is emerging that HAP deposition may play a role in the development and progression of age‐related macular degeneration in the retina and neurodegeneration in the brain.7 Therefore, monitoring calcification in health and disease is critical for diagnosis, monitoring progression and treatment.

There are several methods used to monitor <span class="Disease">calcification, some applicable in vivo while others only work in vitro.10, 11 A number of radiological techniques have the potential to detect <span class="Disease">calcification using radiography,12, 13 fluoroscopy,13 conventional computed tomography (CT),14 electron‐beam tomography (EBT),15, 16 multi‐detector CT,17, 18 intravascular ultrasound,19, 20 magnetic resonance imaging (MRI),21 and transthoracic and transesophageal echocardiography.22 However, most current methods cannot resolve smaller than millimeter sized mineralization and are usually invasive, costly and not well tolerated.23 In vitro, the resolution can be significantly increased: The classic Von Kossa histochemical method relies on silver precipitation at sites of phosphate deposition,24 while Alizarin Red S, a colorimetric label, is widely used to detect calcium deposition.25 In combination these are effective, inexpensive and widely used methods to detect calcium phosphate mineralization in fixed cells in culture or postmortem tissue sections, but they are not very sensitive and subcellular resolution is limited. Fluorescent probes broadly offer better sensitivity than colorimetric ones, but existing stains such as Alizarin Red S, Xylenol Orange, or uranium have clear drawbacks such as modest selectivity among mineral phases, pH dependence, overlap of their fluorescence with tissue autofluorescence. Frangioni and Kovar's research groups developed the second generation fluorescent probes coupling HAP‐binding moieties such as bisphosphonate or tetracycline with red and near‐infrared penta‐ or hepta‐methine cyanine fluorescent moieties; the longer wavelength excitation and emission of these fluorophores substantially reduces scattering and background fluorescence.26, 27, 28 These probes were sensitive, selective, and usable in vivo in animal models, but are costly and by comparison with other probes that exhibit significant or unique changes in fluorescence when binding to particular targets such as DNSA (dansylamide) with carbonic anhydrase,29 the triphenyl methane dye Auramine O with LADH (horse liver alcohol dehydrogenase) with,30 or ethidium bromide with DNA,31 their fluorescence is insensitive to whether they have bound to the (calcified) target or nonspecifically to something else. To address this latter issue, we sought to develop the third generation of fluorescent probes of calcification bearing phosphonic acid metal binding units which are bonded to one of the sp2 carbon atoms of the fluorescent cores, with the goal of differentially perturbing the fluorescence of the probe when bound to calcified substrates, and thereby providing additional information. The use of such fluorophores would be important with respect to generating synergic interactions between the fluorescent core and the d orbitals of the target divalent metal ions.

In this sense, the <span class="Chemical">phosphonic acid <span class="Chemical">metal binding group has recently attracted significant attention in diverse scientific fields ranging from material science to medicine.32, 33 Our initial toxicity studies with aromatic phosphonic acids and phosphonate metal‐organic solids were promising for their in vivo applications inasmuch as ‐H exhibited no toxicity for an intestinal cell line at high concentrations.34, 35 One of the unexplored properties of phosphonic acid metal binding groups is their potential role in imaging metal deposits in living systems. Our and Demadis’ recent work, and Martell's early work from the 1970s all indicate that phosphonates exhibit high affinity towards alkali and alkaline earth metal ions, as well as divalent transition‐metal ions.35, 36, 37, 38, 39 In addition, the pKa2 of phenylphosphonic acid (PhPO3H2) is 7.44, giving PhPO3 2− a −2 charge under physiological pH.40 Therefore, the use of phosphonic acid metal‐binding unit(s) to target biologically significant divalent metal ions offers highly sensitive and pH‐independent metal probes working near physiological pH. Bisphosphonates have been previously attached to cyanine (Osteosense®) and fluorescein moieties with long aliphatic hydrocarbon side chains to label target calcification with green or near infrared fluorescence.39, 41 The presence of sp3 bonds in the aliphatic linker chain in these examples between the phosphonic acid and the fluorescent core in these examples merely used bisphosphonates as recognition moieties and minimized any electronic interactions between the fluorescent core and the phosphonic acid metal binding unit. Therefore, such fluorescent labels provide little if any change in fluorescence intensity upon HAP binding.39, 41, 42, 43 By comparison, the direct conjugation of phosphonic acid metal binding group with an sp2 carbon atom of the fluorescent core extends the conjugation of the fluorescent core up to the coordinated metal ion. Thus, it offers the prospect of the metal‐ion binding the phosphonate and affecting the fluorescence in useful ways. For instance, such binding and recognition of a metal ion might cause useful changes in fluorescence that might help discriminate metal‐bound fluorophores from unbound or non‐specifically bound fluorophores. Such fluorescent phosphonates containing direct sp2 conjugation with the fluorescent core have not been reported in the literature, perhaps due to synthetic difficulties and the high energy requirement to form P−C bonds. Our recent research efforts with arylphosphonic acid synthesis have generated novel strategies to introduce phosphonic acid around aromatic scaffolds, by Suzuki cross coupling or the d‐catalyzed Arbuzov reaction.44, 45, 46, 47

For this study, as seen in Scheme 1, we have synthesized 4 fluorescent probes. Two of them incorpo<span class="Species">rate <span class="Chemical">phenylphosphonic acid as the HAP binding unit with highly conjugated porphyrin cores, namely 5,10,15,20‐tetrakis[p‐phenylphosphonic acid]porphyrin ( ‐H) and 5,10,15,20‐tetrakis[m‐phenylphosphonic acid]porphyrin ( ‐H) (Figure 1; please see the Supporting Information for synthesis details). ‐H has four para‐positioned PPA units promoting direct conjugation between the HAP and the fluorescent core. On the other hand, ‐H has four meta‐positioned PPA units creating a more protective environment between the fluorescent porphyrin core and the HAP. We then explored their potential for binding hydroxyapatite. As a control group we used the isopropyldiester and ethyldiester analogues of ‐H and ‐H, namely ‐H and ‐H (see the Supporting Information for detailed synthesis). A previous synthesis of ‐H relied on the Ni‐catalyzed Arbuzov reaction.48 Therefore, ‐H that is synthesized using this route usually has Ni bound to the nitrogens in the porphyrin core. In this study, we have used an alternative method using Pd‐catalyzed Arbuzov reaction to obtain metal free ‐H. (please see the Supporting Information for synthesis details, NMR, FTIR spectra, and the crystallographic tables).

Scheme 1

The fluorescent probes used in this study: A) 5,10,15,20‐Tetrakis[p‐(diisopropoxyphosphoryl)phenyl]porphyrin ( ‐H). B) 5,10,15,20‐Tetrakis [p‐phenylphosphonic acid]porphyrin ( ‐H). C) 5,10,15,20‐Tetrakis[m‐(diethoxyphosphoryl)phenyl]porphyrin ( ‐H). D) 5,10,15,20‐Tetrakis [m‐phenylphosphonic acid]porphyrin ( ‐H).

Figure 1

Mouse ribs incubated with either ‐H (λ ex/em 595/613 nm; exposure time −200 ms) or ‐H (λ ex/em 578/603 nm; exposure time −100 ms) diluted to 1 mg mL−1 in HEPES (A–E or F–J, respectively) and counter‐stained with DAPI (λ ex/em 359/461 nm; exposure time: −200 or 100 ms, respectively). Images were captured on the day of staining (A and F), as well as after 4 days (B and G), 7 days (C and H), and 14 days (D and I). A negative control of mouse ribs incubated with each buffer alone is also included (E and J, respectively). Scale bar=100 μm.

The fluorescent probes used in this study: A) 5,10,15,20‐Tetrakis[p‐(diisopropoxyphosphoryl)phenyl]<span class="Chemical">porphyrin ( ‐H). B) 5,10,15,20‐Tetrakis [p‐<span class="Chemical">phenylphosphonic acid]porphyrin ( ‐H). C) 5,10,15,20‐Tetrakis[m‐(diethoxyphosphoryl)phenyl]porphyrin ( ‐H). D) 5,10,15,20‐Tetrakis [m‐phenylphosphonic acid]porphyrin ( ‐H).

<span class="Species">Mouse ribs incubated with either ‐H (λ ex/em 595/613 nm; exposure time −200 ms) or ‐H (λ ex/em 578/603 nm; exposure time −100 ms) diluted to 1 mg mL−1 in <span class="Chemical">HEPES (A–E or F–J, respectively) and counter‐stained with DAPI (λ ex/em 359/461 nm; exposure time: −200 or 100 ms, respectively). Images were captured on the day of staining (A and F), as well as after 4 days (B and G), 7 days (C and H), and 14 days (D and I). A negative control of mouse ribs incubated with each buffer alone is also included (E and J, respectively). Scale bar=100 μm.

To probe their <span class="Chemical">HAP binding properties in a biological matrix, we have used cross sectioned <span class="Species">mouse ribs as an example for naturally occurring HAP. The sections were incubated with ‐H ‐H ‐H at concentrations ranging from 0.01 to 1.0 mg mL−1 in HEPES buffer for varying times at room temperature, then imaged by fluorescence microscopy (details below in the figure legends), to assess HAP binding capability. Ribs incubated with 1 mg mL−1 ‐H showed a greater fluorescence intensity than both 0.1 mg mL−1 and 0.01 mg mL−1 (Figure S17 A–C, respectively), whilst still showing clear fluorescence signal at the lowest concentration of 0.1 mg mL−1 used here.

This indicates that the dye binding to <span class="Chemical">HAP is concent<span class="Species">ration dependent. When the mouse ribs were incubated with 1 mg mL−1 ‐H in HEPES for differing times from 120 to 10 mins (Figure S18 A–E), there was a clear decrease in fluorescence intensity but even the 10 min short incubation yielded an appreciable fluorescence compared to the negative control (Figure S18 E compared to Figure S18 F). When ribs were incubated with ‐H diluted to 1 mg mL−1 in different buffers, there was no clear difference between the fluorescence intensity of HEPES, PBS, TBS (Figure S19 A–C, respectively). However, when ‐H was diluted in dH2O (Figure S19 D), there was no fluorescent signal observed. Sections were re‐imaged at several time points after the original microscopy sessions to observe the stability of labeling. There was a noticeable decrease in fluorescence intensity in all of the solvents although signal diminished faster in HEPES buffer than in PBS or TBS (Figure S20). At the two week time point there was still a weak fluorescent signal observed for ‐H diluted in PBS, but not for the other buffers (Figure S20 N compared to Figure S20 M, O and P). No signal was associated with incubating the ribs with the solvents as a negative control (Figure S20 Q‐T)

The <span class="Chemical">phosphonic acid moieties in ‐H are more protected compared to the para‐positioned ‐H. When <span class="Species">mouse ribs were incubated with different concentrations of ‐H, (1 to 0.01 mg mL−1 in HEPES buffer) we found little to no difference in the fluorescence intensities (Figure S21 A–C, respectively). When the mouse ribs were incubated with 1 mg mL−1 ‐H in HEPES for differing times, 10 to 120 mins, there were no appreciable difference in fluorescence intensities at the different incubation times (Figure S22 A–E, respectively) while the fluorescent intensities were clearly distinguishable from HEPES alone (Figure S22 F). Imaging of the sections were repeated two weeks following the original microscopy and we found no noticeable decrease in fluorescence intensity between ribs incubated with 1 mg mL−1 ‐H in HEPES buffer and imaged on the day of staining compared with images taken 4, 7 and 14 days later (Figure 1 F–I, respectively). This is a noticeable difference compared to ‐H, with a less protected structure, where there is a loss of fluorescent signal with increasing time after initial staining (Figure 1 A–D, respectively). This could be associated with the more protected HAP phosphonic acid interaction in the meta position limiting the interactions with the surrounding molecules buffers etc. Again, no signal was associated with incubating the ribs with HEPES only as a negative control (Figure 1 E and I, respectively).

As seen in Figure 2, the absorbance peak (Figure 2 A) of ‐H in <span class="Chemical">PBS, <span class="Chemical">TBS and HEPES with the addition of HAP corresponds with the absorbance of the dye in d‐DMSO (Figure S16). There is a noticeable shift in the absorbance peak maximum when diluted in d H2O, from 415 nm to 435 nm, which suggests a shift in the fluorescent properties of the dye due to protonation. This is also reflected in the maximal peak of the fluorescence intensity (Figure 2 B), with a shift from λ em 646–648 nm for PBS, TBS and HEPES to λ em 675 nm when diluted in dH2O. The fluorescence intensity of ‐H is also substantially increased by 1.8‐, 2.0‐, 2.0‐, and 1.6‐fold upon HAP binding of the fluorescent probe ‐H in PBS, TBS, HEPES and d H2O, respectively (Figure 2 B, solid vs. dashed lines). Previously reported bisphosphonate fluorophores had sp3 aliphatic carbons between the fluorescent core and HAP binding, therefore, such systems merely functioned as fluorescent labels with no change in emission due to HAP binding since they lacked synergistic interaction between the HAP and the fluorescent core. Phosphonic acids that have direct sp2 bonds to the fluorescent core could extend the conjugation of the fluorescent core to the HAP and thereby could initiate changes in the ground and excited states resulting in quenching or enhancing the fluorescence emission. As seen in Figure 2 (B), upon binding of HAP, ‐H produces increased fluorescence supporting this hypothesis; ‐H is thus the first example of a single sp2 bonded phosphonic acid unit targeting HAP in the literature.

Figure 2

The absorbance (A) and fluorescence (B) spectra of 0.01 mg mL−1 ‐H in the presence (dashed lines) and absence (solid lines) of HAP. The dye was diluted to 0.01 mg mL−1 in PBS (pH 7.4, green), TBS (pH 7.4, orange), HEPES (pH 7.4, purple) and d H2O with absorbance and fluorescence spectra obtained using the Flexstation 3 microplate reader.

The absorbance (A) and fluorescence (B) spectra of 0.01 mg mL−1 ‐H in the presence (dashed lines) and absence (solid lines) of <span class="Chemical">HAP. The dye was diluted to 0.01 mg mL−1 in <span class="Chemical">PBS (pH 7.4, green), TBS (pH 7.4, orange), HEPES (pH 7.4, purple) and d H2O with absorbance and fluorescence spectra obtained using the Flexstation 3 microplate reader.

Comparable experiments with <span class="Species">mouse rib sections were conducted using the <span class="Chemical">isopropyldiester forms ‐H and ‐H (See Scheme 1 a and 1 c) as stains. We found a complete lack of HAP‐associated staining with these compounds suggesting that the interaction of phosphonates with HAP was reduced by the isopropylester groups on the phosphonates, preventing binding and interaction of the fluorescent porphyrin core with the HAP. We also noted that the presence of hydrophobic isopropyl groups dramatically reduced their solubilities in the aqueous.

Aiming to use <span class="Chemical">phenylphosphonic acid functionalized <span class="Chemical">porphyrins in in vivo applications, the negative charge on the deprotonated phosphonate might be a handicap by limiting cell permeability. Optional demasking of phosphonate esters in metabolic surroundings might occur, recreating the metal binding PhPO3 2−. This possibility led us to examine ‐H and ‐H suitability for in vivo cellular experiments by testing their permeability on proliferating human THP‐1 monocytes. The cells were probed with either ‐H or ‐H in a HEPES‐based buffer containing 0.3 % bovine serum albumin. Albumin binds a wide variety of hydrophobic ligands under physiological conditions, so we assumed an improved solubility/accessibility for the isopropyl diester molecule for cellular uptake. In addition, albumin is a regular component of culture media.

As seen in Figure 3, the fluorescence spectra of ‐H‐loaded THP‐1 cells very much resembles the characteristics of the sensor diluted in <span class="Chemical">HEPES‐buffer (see Figure 1 A, F). Thus, beyond the low <span class="Disease">toxicity ‐H provides two more positives ‐cell permeability and cellular retention‐ desirable for imaging applications. ‐H was much less efficient in labeling the THP‐1 cells (see Figure S23). We hypothesize that the phenylphosphonic acid porphyrins, being somewhat amphipathic, were able to penetrate the cell membrane, whereas the more nonpolar esters were not as efficient.

Figure 3

Fluorescence spectra of THP‐1 monocytes cells incubated with ‐H.

In conclusion, herein, we have reported next‐gene<span class="Species">ration fluorescent probes to target calcifications, namely ‐H, ‐H, ‐H, and ‐H, in which the phosphonic acid metal binding unit(s) are exclusively bonded to sp2 carbon atoms of the fluorescent core. sp2 bonding of the metal binding unit to the fluorescent core further extended the conjugation of the fluorescent core to the HAP, leading to significant increase in fluorescence upon HAP binding. We further used these fluorescent probes to target the HAP in mouse ribs and observed their interaction with human cells. Both ‐H and ‐H have shown HAP specific binding in rat bone sections. The more protected metal binding nature of the ‐H resulted in longer fluorescence period compared to its positional isomer ‐H. As a control, we have also synthesized phosphonatediesters of the synthesized fluorescent probes, which showed no HAP binding. ‐H can travel through the cellular membrane, whereas the presence of bulky and hydrophobic isopropyl groups in ‐H hindered their passage through the cellular membrane. This is the first study utilizing sp2‐bonded phosphonic acids with the fluorescent cores to target HAP mineralizations. We have shown that compact fluorescent probes with phosphonic acid metal binding group(s) may be used to monitor microcalcifications and calcifications. In addition, their easy acceptance into the cellular matrix indicate that they could be used to target organelle‐specific calcifications such as mitochondrial calcifications. The reported low toxicity of ‐H and the new synthetic methods indicate that they can be used in targeting wide range of calcifications in vivo. We are currently developing our library to target organelle specific calcifications.

Animal Experiments

Animal procedures were approved by Queen′s University Belfast Animal Welfare and Ethical Review Body (AWERB) and authorized under the UK Animals (Scientific Procedures) Act 1986. Animal use conformed to the standards of the ARVO Statement for the Use of Animals in Ophthalmic and Vision Research and with European Directive 210/63/EU.

Conflict of interest

G.Y. and H.H. have pending patent protecting some of the presented data.

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Supplementary

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