Calcium Dyshomeostasis Alters CCL5 Signaling in Differentiated PC12 Cells

Radzik, Tomasz; Boczek, Tomasz; Ferenc, Bozena; Studzian, Maciej; Pulaski, Lukasz; Zylinska, Ludmila

doi:https://doi.org/10.1155/2019/9616248

BioMed Research International

On this page

Abstract Introduction Materials and Methods Results Discussion Conclusions Data Availability Conflicts of Interest Authors’ Contributions Acknowledgments References Copyright Related Articles

Research Article | Open Access

Volume 2019 | Article ID 9616248 | https://doi.org/10.1155/2019/9616248

Calcium Dyshomeostasis Alters CCL5 Signaling in Differentiated PC12 Cells

Tomasz Radzik,¹Tomasz Boczek,^1,2Bozena Ferenc,¹Maciej Studzian,³Lukasz Pulaski,^3,4and Ludmila Zylinska¹

Guest Editor: Hailong An

Received11 Jan 2019

Accepted04 Mar 2019

Published26 Mar 2019

Abstract

Background. Plasma membrane Ca²⁺-ATPase (PMCA) is the most sensitive cellular calcium detector. It exists in four main isoforms (PMCA1-4), among which PMCA2 and PMCA3 are considered as fast-acting neuron-specific forms. In the brain, PMCA function declines progressively during aging; thereby impaired calcium homeostasis may contribute to some neurodegenerative diseases. These destructive processes can be propagated by proinflammatory chemokines, including chemokine CCL5, which causes phospholipase C-mediated liberation of Ca²⁺ from endoplasmic reticulum by IP₃-gated channels. Methods. To mimic the changes in aged neurons we used stable transfected differentiated PC12 cells with downregulated PMCA2 or PMCA3 and analyzed the effect of CCL5 on calcium transients with Fluo-4 reagent. Chemokine receptors were evaluated using Western blot, and IP₃ receptors expression level was assessed using qRT-PCR and Western blot. Results. In PMCA-reduced cell lines, CCL5 released more Ca²⁺ by IP₃-sensitive receptors, and the time required for Ca²⁺ clearance was significantly longer. Also, in these lines we detected altered expression level of CCR5 and IP₃ receptors. Conclusion. Although modification of PMCAs composition could provide some protection against calcium overload, reduction of PMCA2 appeared to be more detrimental to the cells than deficiency of PMCA3. Under pathological conditions, including inflammatory CCL5 action and long-lasting Ca²⁺ dyshomeostasis, insufficient cell protection may result in progressive degeneration and death of neurons.

1. Introduction

Growing body of evidence suggests that disrupted calcium homeostasis plays a detrimental role in triggering neurodegeneration. This process can also be propagated by repeated inflammatory reactions, including local production of chemokines. These events intensify particularly during aging, when the proper response to extracellular signals is decreased due to accumulation of multiple cellular damage and pathologies [1–4]. Injured cells are exposed to a prolonged elevation of intracellular Ca²⁺ that in turn initiates a number of abnormal processes, which can finally lead to cell death [5–7]. Disturbances in calcium homeostasis have been attributed to imbalance between calcium “on” and “off” systems, which affects cell survival. In healthy cells, the first step in decreasing cytosolic Ca²⁺ relies on three modes: uptake into endoplasmic reticulum by sarco/endoplasmic Ca²⁺-ATPase (SERCA), extrusion by high-capacity but low-affinity Na⁺/Ca²⁺ exchanger (NCX), and removal by plasma membrane Ca²⁺-ATPase (PMCA) [8, 9]. The latter is the most sensitive element with low capacity, but very high affinity. The enzyme is represented by 4 main isoforms with ~30 variants that exhibit differential spatial and developmental expression pattern [10, 11]. The two ubiquitous isoforms, PMCA1 and PMCA4, are far less effective in controlling calcium homeostasis than the two neuron-specific PMCA2 and PMCA3 isoforms. The expression profile of PMCAs changes significantly during development, reflecting the specific function of each isoform. Changes in PMCA expression and activity have also been reported during aging. It is believed that PMCA loss may significantly impair calcium extrusion in senescence neurons making them more susceptible to neurotoxic insults [12–17]. Ca²⁺-mediated neurotoxicity has been shown for several neurodegenerative diseases including Alzheimer’s disease (AD), Huntington disease (HD), spinocerebellar ataxias (SCAs), Parkinson’s disease (PD), schizophrenia, or bipolar disorder [6, 15, 18–22].

Additional factors contributing to neuronal death are inflammatory mediators, including some chemokines [1, 23]. Among 50 discovered chemokines, chemokine C-C motif ligand 5 (CCL5, RANTES) is of particular interest due to its potential role as a modulator of cellular metabolism and brain architecture [23–25]. CCL5 is constitutively expressed in the adult central nervous system, with region-specific expression pattern [26]. A remarkable increase of CCL5 in central nervous system (CNS) can be detected during permeabilization of the blood–brain barrier and after extensive production of CCL5 from astrocytes and microglial cells, triggered by proinflammatory factors [27–31]. One of the mechanisms of action of CCL5 is a positive control of cytosolic Ca²⁺ mobilization after binding to three receptors: CCR1, CCR3, and CCR5 [23, 32]. They are cell surface–associated, immune-regulatory G protein–coupled receptors (GPCRs). CCL5 binding activates a G protein, which subsequently activates phospholipase C (PLC) involved in a second messenger system. PLC-mediated hydrolysis of phosphatidylinositol 4,5-bisphosphate (PIP₂) gives rise to two products: 1,2-diacylglycerol and inositol 1,4,5-triphosphate (IP₃). IP₃ stimulates the release of Ca²⁺ from intracellular stores through IP₃ receptors, which exist in three different isoforms [33–35].

The present study was undertaken to clarify the potential role of CCL5-mediated signaling using the model of differentiated PC12 cells, which is one of the most frequently used models for studying neuronal processes. We have previously developed stable transfected lines of PC12 cells with downregulated expression of neuron-specific PMCA2 (_2 line) or PMCA3 (_3 line), which have been validated in our several other studies [36, 37]. The most critical finding was permanently increased resting cytosolic Ca²⁺ concentration in PMCA-reduced lines due to compromised Ca²⁺ extrusion ability observed even despite compensatory stimulation of PMCA1 expression detected in both lines and of PMCA4 in _3 line [36]. We have also provided the evidence that altered PMCA composition may play a role in regulation of bioenergetic function of mitochondria [37, 38]. Moreover, PMCA altered expression of genes encoding a number of elements responsible for regulation of calcium homeostasis [39, 40]. Taking into consideration that decreased amount and activity of PMCA may underlie many neurodegenerative diseases, here we analyzed whether the modified profile of plasma membrane calcium pumps can influence cell response to CCL5-induced signaling.

2. Materials and Methods

2.1. Cell Culture

Cell culture and differentiation PC12 rat pheochromocytoma cells (ATCC, USA) were routinely maintained in RPMI-1640 medium (Biowest, USA) containing 15% fetal bovine serum (Biowest, USA), 25 mM HEPES, pH 7.4 (21°C), 2 mM L-glutamine, 25 U/ml penicillin, and 25 μg/ml streptomycin in a humidified incubator at 37°C with 5% CO₂. Stable transfected cell lines with reduced PMCA2 (_2) or PMCA3 (_3) protein level were achieved using an antisense RNA cloned into pcDNA3.1(+) vector transfected to naive PC12 cells, as described previously [36]. Following selection with increasing G418 concentration (up to 1 mg/ml), the stable transfectants with nearly 50% reduction in PMCA2 or PMCA3 protein level were obtained. PC12 cells carrying an empty vector were used as a control (C). PC12 cells derived from a transplantable rat pheochromocytoma can differentiate into sympathetic-like neuronal cells upon exposure to neurotrophins, but similar effects can be triggered by db-cAMP. In our model differentiation process was induced with 1 mM dibutyryl-cAMP (Santa Cruz Biotechnology) for 48 h. Because PC12 cells exhibit some level of variability, routinely no more than 12 passages were used.

2.2. Ca²⁺ Measurement

Cells grown to 80% confluence in 25 cm² flasks were detached from the surface and centrifuged at low speed (250 × g) for 5 min. 100 μl of cell suspension was immediately transferred to 96-well plates. An equal volume of 2× concentrated Fluo-4 Direct calcium reagent loading solution (Life Technologies, USA) was added to each well and plates were incubated at 37°C for 1 h. Fluorescence was measured by using a Victor X3 plate reader (Perkin-Elmer). The measurements were performed for 250 s at one second intervals at 37°C and the fluorescence signal was recorded using 488 nm excitation filter and 535 nm emission filter. The signal was calibrated by addition of 0.1% Triton X-100 to obtain and 10 mM EGTA to chelate extracellular Ca²⁺ to obtain . Appropriate controls for estimation of background fluorescence including phenol red free RPMI medium, Fluo-4 solution alone, and cell-free recording solution were included. Changes in fluorescence of Fluo-4 dye were converted to free cytosolic Ca²⁺ concentration according to the equation = ([F-]/[-F]), where = 345 nM. All measurements were performed in a calcium-free buffer containing 125 mM NaCl, 5 mM KCl, 1.2 mM KH₂PO₄, 1.2 mM MgSO₄, 6 mM glucose, and 25 mM HEPES. In all experiments, after measurement of basal Ca²⁺ for 150 s, 50 ng/ml of CCL5 (PeproTech) was added. For analysis of CCR/PLC/IP₃R pathway, specific inhibitors were added right before measurements—cocktail of CCRs inhibitors: 1 nM BX513 (Abcam) for CCR1, 1 μM SB328437 (Abcam) for CCR3 and 1 nM DAPTA (Abcam) for CCR5 or 4 μM U73122 (Abcam) for PLC, or 100 μM 2-APB (Sigma) for IP₃Rs. To determine the role of ER calcium stores in CCL5 response, 1 μM thapsigargin (Santa Cruz Biotechnology) was added 50 s after basal calcium measurement, and next 50 ng/ml of CCL5 at 150 s was applied. All measurements were done in duplicate and the data presented in the figures are the average of at least 5 independent cell cultures.

2.3. RNA Isolation and Real-Time PCR

Total cellular RNA was isolated using Tri Reagent (MRC) according to the manufacturer’s protocol. 1 μg of purified RNA and oligo(dT) primers were then used for cDNA synthesis using High-Capacity cDNA Reverse Transcription Kit (Applied Biosystems). The IP₃R genes expression level was quantified in a real-time PCR reaction using 5x HOT FIRE Pol Eva Green qPCR Mix Plus (Solis Biodyne) in the following conditions: 15 min at 95°C followed by 40 cycles at 95°C for 15 s, 60°C for 30 s, and 72°C for 30 s using ABI Prism 7000 sequence detection system (Applied Biosciences). Following normalization to the expression of endogenous Gapdh, the fold change of each target gene was calculated using comparative method as described previously [36]. Primers were synthesized in the Institute of Biochemistry and Biophysics (Poland) and their specificity was confirmed by running a melting curve after each reaction. Primers were designed using GenScript Primer Design Tool (USA) and their sequences were as follows:

Ip3r-1 forward: 5′-GTGGAGGTTTCATCTGCAAGC-3′, reverse: 5′-GCTTTCGTGGAATACTCGGTC-3′,

Ip3r-2 forward: 5′-GCTCTTGTCCCTGACATTG-3′, reverse: 5′-CCCATGTCTCCATTCTCATAGC-3′,

Ip3r-3 forward: 5′-AGCGAGAAGCAGAAGAAAG-3′, reverse: 5′-CATCCGTGGGAACCAGTC-3′,

Gapdh forward: 5′-GCTTACCAG-GGCTGCCTTCT-3′, reverse: 5′-CTTCCCATTCTCAGCCTTGAC-3′.

2.4. Western Blotting

Approximately 40-80 μg of cell lysate proteins were separated using either 8% or 10% SDS-PAGE and electroblotted onto nitrocellulose membranes using semidry method. The membranes were blocked with 3% BSA in TBS buffer (10 mM Tris–HCl, pH=7.4, 150 mM NaCl) for 30 min at room temperature prior to exposure to primary antibodies. Membranes were incubated overnight at 4°C with the primary antibodies and for approximately 4 h with the secondary antibodies at room temperature followed by 3 × 15 min wash with TBS-T between each antibody application. The following primary antibodies were used: anti-CCR1 (rabbit, polyclonal, 1:1000, Santa Cruz Biotechnology; rabbit, polyclonal, 1:1000, BosterBio), anti-CCR3 (rabbit, polyclonal, 1:1000, Santa Cruz Biotechnology; rabbit, monoclonal, 1:1000, BosterBio), anti-CCR5 (mouse, monoclonal, 1:1000, Santa Cruz Biotechnology), anti-IP₃R-1 (rabbit, polyclonal, 1:2000, Alomone Labs), anti-IP₃R-2 (rabbit, polyclonal, 1:200, Alomone Labs), monoclonal anti-IP₃R-3 (mouse, monoclonal, 1:2000, BD Biosciences), and anti-IP₃R-1/2/3 (mouse, monoclonal, 1:500, Santa Cruz Biotechnology). Monoclonal anti-β-actin antibody (Santa Cruz Biotechnology) was used at 1:1000 dilution as a protein loading control. Secondary antibodies coupled with alkaline phosphatase (Sigma) at 1:5000 dilution were used for staining. Sigma Fast BCIP/NBT was used for visualization according to the manufacturer’s instruction. Blots were scanned and band intensities were measured quantitatively using GelDoc™ EQ system with Quantity One 1-D Analysis Software version 4.4.1 (Bio-Rad).

2.5. Confocal Imaging

Cells were seeded at a density of 2 × 10⁴ cells/well on thin-glass bottomed 96-well plate (SensoPlate™, Greiner Bio-One) and differentiated for 48 h. Next, cell cultures were washed once with PBS and fixed for 10 min in room temperature with 2% formaldehyde freshly prepared from paraformaldehyde and buffered to pH = 7.4 in PBS. Subsequently, cells were washed once and further incubated for 1 h with the blocking buffer (10% normal goat serum, 0.1% Triton X-100, PBS pH = 7.4), following 1 h incubation with primary antibody against CCR5 diluted in the blocking buffer (1:100, Santa Cruz Biotechnology). Next, cells were washed 3 × 5 min with the blocking buffer and incubated for 1 h with secondary goat anti-mouse IgG1 antibody conjugated with Alexa Fluor 488 (1:1000, Thermo Fisher Scientific) to fluorescently label immunodetected CCR5. Subsequently, after 3 × 5 min wash with the blocking buffer, plasma membrane marker protein Na⁺/K⁺ ATPase was immunostained for 1 h with primary antibody (Abcam) fluorescently labeled with Zenon™ Alexa Fluor 568 Mouse IgG1 Labeling Kit (Thermo Fisher Scientific) and diluted in the blocking buffer (1:50). Finally, cells were washed 3 × 5 min with the blocking buffer, once with PBS, and were fixed again for 10 min in room temperature with 2% formaldehyde in PBS (pH = 7.4). Eventually, cell nuclei were counterstained with 5 μM Hoechst 33342 in PBS, and triple-stained cells were visualized by confocal microscopy. Images were obtained using 780 LSM confocal microscope (Zeiss) with Plan-Apochromat 63x/1.4 Oil DIC M27 objective. ZEISS Microscope Software ZEN2012 was used to calculate mean fluorescence intensities of respective CCR5-positive pixels colocalizing with plasma membrane marker (Na⁺/K⁺ ATPase-positive) pixels. Plasma membrane marker-positive pixels were selected based on their fluorescence intensity that ought to be between arbitrary upper (500 units) and lower (40 units) thresholds, set either to eliminate nonspecific background staining or to negate the influence of high-intensity artificial staining (antibody precipitates and others). Analysis of fluorescence intensity of CCR5 staining colocalizing with plasma membrane staining was performed for each cell line for five different fields of view and results were averaged.

2.6. Data Analysis

The data are shown as means ± SD of n separate experiments (n ≥ 3) with the exact n value given under each figure. The comparisons between cell lines were done using Student’s t-test or ANOVA followed by Tukey or Bonferroni’s multiple comparisons tests, wherever applicable. P values were calculated using STATISTICA 12.0 (StatSoft) or GraphPad Prism 7 (GraphPad, La Jolla, CA). P < 0.05 was considered as statistically significant.

3. Results

3.1. CCRs Expression in PC12 Cell Lines

First, we evaluated the presence of CCR1, CCR3, and CCR5 in PC12 lines using two approaches. The immunoreactivity of examined receptors was initially assayed in a cell lysate by Western blot (Figure 1). In comparison to the control cells, CCR1 was present at higher level in _3 cells, CCR3 increased in _2 cells, but in both PMCA downregulated PC12 lines CCR5 amount increased by nearly 50%.

Figure 1

Western blot analysis of CCRs protein in PC12 cell lines. (a) Approximately 40–60 μg of total protein was resolved on a 10% SDS-PAGE gel and electroblotted onto nitrocellulose membranes. Membranes were probed with polyclonal anti-CCR1, polyclonal anti-CCR3, or monoclonal anti-CCR5. Representative blots are shown and arrows indicate the main band of the receptors with apparent MW 41 kDa for CCR1, 40 kDa for CCR3, and 46 kDa for CCR5. (b) The bands intensity was densitometrically analyzed and the results are expressed as % of the control PC12 cells obtained after normalization to endogenous β-actin level (± SD). P < 0.05 (n=7), C: control line, _2: PMCA2-reduced line, _3: PMCA3-reduced line.

Since functionally active chemokine receptors are located at the plasma membranes, we next explored cellular distribution of CCRs by confocal microscopy. Staining of endogenous CCR1 and CCR3 showed low immunosignal intensity, which was concentrated predominantly in the cytosolic area (data not shown). To validate these results, we repeated the assay using another set of antibodies against CCR1 and CCR3; however, we obtained similar results. These data indicated that although CCR1 and CCR3 were present in PC12 cell lines, their participation in CCL5 signaling in our model seems to be negligible. CCR5 was expressed much more abundantly and was mostly distributed in the plasma membranes (Figure 2). Quantification of CCR5 immunofluorescence revealed that cells with reduced PMCA2 or PMCA3 contained more plasma membrane-located receptor than that of control line.

Figure 2

Localization of CCR5 in PC12 cell lines. PC12 cells differentiated for 48 h with db-cAMP were fixed and immunostained with antibodies against CCR5 receptor (green) and Na⁺/K⁺ ATPase (plasma membrane marker, red). Nuclei were stained with Hoechst 33342 (blue). Representative confocal images are presented. Values shown in merged images represent average fluorescence intensity ± SEM (n = 5) of pixels positive in green channel (CCR5) that colocalize with red channel positive pixels (Na⁺/K⁺ ATPase). P< 0.05, P < 0.01. Scale bars: 10 μm. C: control line, _2: PMCA2-reduced line, _3: PMCA3-reduced line.

3.2. CCL5 Effect on Calcium Transients

To analyze CCL5-induced cytosolic Ca²⁺ increase in examined PC12 cell lines, chemokine action was assayed in a calcium-free medium to avoid the secondary effect triggered by “calcium-induced calcium release” process, as well as the concomitant participation of membrane calcium channels. Changes in fluorescence were monitored for 250 s at one-second intervals, and CCL5 was always applied after 150 s of measurement. The CCL5 concentration was chosen because it was shown to be effective under inflammatory state, which is supported by literature data. It is also frequently used for in vitro assays including PC12 cells [41]. At resting state higher Ca²⁺ level in PMCA-reduced PC12 cells was observed (Figure 3), confirming our previous results [36].

Treatment with CCL5 at 50 ng/ml increased cytosolic Ca²⁺ in all examined lines, more intensively in PMCA-modified cells, but the highest peak value was observed in _2 line. This was also confirmed by analysis of area under the curves. Time course of chemokine effect presented in Figure 4(a) (black lines) showed a fast transient increase in [Ca²⁺ during first seconds after CCL5 application, followed by a slow, progressive decrease in [Ca²⁺. The estimated time required for recovery of Ca²⁺ to the basal level was 14 ± 1 s for control PC12 cells, 41 ± 8 s for _2 line, and 23 ± 7 s for _3 line (n=5; P < 0.05 vs. control; ^#P < 0.05 _3 vs. _2). Slower recovery in _2 and _3 lines could result from lowered Ca²⁺-clearing potency in PMCA-reduced lines, since SERCA affinity for calcium is at low micromolar range [42]. In Ca²⁺-free conditions, the differences in cell response to CCL5 might reflect a balance between intensity of Ca²⁺ release from ER and Ca²⁺ extrusion, which varied between cell lines.

(a)

(b)

Figure 4

Analysis of CCL5 effect on calcium transients in PC12 cell lines. Ca²⁺ transients were measured in parallel wells with (red lines) or without (black lines) presence of specific inhibitors. (a) SERCA inhibitor, 1μM thapsigargin, was added after 50 s (red arrow), and next 50 ng/ml CCL5 was applied after 150 s (black arrow). (b) CCRs inhibitors, 1 nM BX513 for CCR1, 1 μM SB328437 for CCR3, and 1 nM DAPTA for CCR5, were included just before measurements. 50 ng/ml CCL5 was applied after 150 s (black arrow). All measurements were done in duplicate and the presented traces are average from 5 independent cell cultures (n=10). C: control line, _2: PMCA2-reduced line, _3: PMCA3-reduced line.

To verify that in our experimental conditions the endoplasmic reticulum was a main source of calcium, the assay was performed in the presence of 1μM thapsigargin added after 50 s, and next CCL5 was applied at 150 s. As shown in Figure 4(a) (red lines), Tg caused a successive calcium depletion from ER due to inhibition of Ca²⁺ reuptake by SERCA, and subsequent addition of chemokine had no effect on calcium transient. To confirm the participation of CCRs in generation of Ca²⁺ transient, the assay was also performed in the presence of specific CCRs inhibitors. Although CCR5 appeared to be the main functionally active receptor in our cell lines, chemokine action was assessed in the presence of cocktail of CCR1, CCR3, and CCR5 inhibitors added just before measurement (Figure 4(b), red lines). CCL5 applied after 150 s did not affect Ca²⁺ level indicating that examined CCRs were indeed the crucial targets for the chemokine.

3.3. Analysis of PLC/IP₃R Pathway

In the next step we analyzed the downstream signaling triggered by CCL5/CCR complex by inhibiting the crucial elements of this pathway, PLC and IP₃ receptors. As shown in Figure 5(a) (red lines), in the presence of selective PLC inhibitor, U73122, there was no Ca²⁺ response to CCL5 in examined cell lines, which confirmed that PLC-induced signaling must be the chemokine effector. Subsequent generation of a second messenger, IP₃, leads to the opening of IP₃-dependent calcium channels. Thus, we treated cells with 2-APB, an inhibitor of IP₃ receptors (Figure 5(b), red lines). Baseline Ca²⁺ level was not affected by the chemokine in these conditions, showing that IP₃Rs were indeed responsible for observed calcium transients.

(a)

(b)

Figure 5

Analysis of PLC/IP₃R signaling pathway in PC12 cell lines. Analysis of PLC/IP₃R pathway was performed in parallel wells with (red lines) or without (black lines) presence of specific inhibitors included just before measurements. 50 ng/ml CCL5 was always applied after 150 s (black arrow). The calcium transients were assayed in the presence of (a) PLC inhibitor, 4μM U73122, and (b) IP₃Rs inhibitor, 100 μM 2-APB. All measurements were done in duplicate and the presented traces are average from 5 independent cell cultures (n=10). C: control line, _2: PMCA2-reduced line, _3: PMCA3-reduced line.

3.4. Characteristics of IP₃ Receptors in PC12 Cell Lines

Since IP₃ receptors appeared to be the final CCL5 effectors in analyzed pathway, we next characterized their expression in our PC12 cell lines. Real-time PCR analysis showed significant IP₃R-1 and IP₃R-2 downregulation in both _2 and _3 lines, whereas the expression of IP₃R-3 increased in comparison to the control cells (Figure 6).

To validate whether the mRNA changes correlated with corresponding receptor protein, Western blot analysis was performed using isoform-specific antibodies and the antibody that recognized all three IP₃ receptors (Figure 7(a)). Single bands of the predicted sizes for IP₃-1, 2, and 3 receptors (~313 kDa, 260 kDa, and 250 kDa, respectively) were detected in all lines, but some lower molecular weight bands were also present. They could represent proteolytic fragments of the receptors, as similar observations were also shown in another study [43].

Figure 7

Western blot analysis of IP₃ receptors in PC12 cell lines. (a) Approximately 60–80 μg of total protein was resolved on an 8% SDS-PAGE gel and electroblotted onto nitrocellulose membranes. Membranes were probed with anti-IP₃R1, anti-IP₃R2, anti-IP₃R3, and recognizing all isoforms anti-IP₃R-T antibodies. Representative blots are shown and arrows indicate the main band of the receptors. (b) Band intensity was densitometrically analyzed and the results are expressed as % (± SD) of control PC12 cells obtained after normalization to endogenous β-actin level. P< 0.05 (n=7). C: control line, _2: PMCA2-reduced line, _3: PMCA3-reduced line.

Quantification of individual IP₃R isoforms confirmed that in _2 and _3 lines the protein level of IP₃R-1 and 2 was lower than that of control cells, but IP₃R-3 increased by ~40% (Figure 7(b)). However, analysis of blots probed with antibody recognizing all IP₃ receptors revealed a total increase only in _3 line. This apparently indicates the differences in a ratio between IP₃R isoforms and finally could result in diversified affinity for IP₃ in both PMCA-reduced cell lines.

4. Discussion

Our previous studies revealed that, in differentiated PC12 cells, downregulation of neurospecific PMCA2 or PMCA3 increased cytosolic Ca²⁺ and subsequently affected the expression level of several Ca²⁺-associated proteins, i.e., SERCA, calmodulin, calcineurin, neuromodulin (GAP43), and certain types of voltage-gated calcium channels [36, 39, 40]. We have also revealed a compensatory increase of PMCA1 isoform in both PMCA-reduced lines coexisting with higher expression of SERCA2 and SERCA3, which correlated with higher Ca²⁺ accumulation in the endoplasmic reticulum [36]. On the one hand it could effectively decrease cytosolic Ca²⁺ concentration to its safe level, but on the other hand, it may potentially increase Ca²⁺ release after activation of calcium channels in the ER, including activation of IP₃ receptors and ryanodine receptors [42]. Since IP₃R-mediated Ca²⁺ release from the ER and mitochondrial Ca²⁺ homeostasis are physiologically coupled, their improper cooperation may significantly affect cell viability [44].

Based on current study, we can add to the list of common features detected after reduction of PMCA2 or PMCA3 increased level of CCR5 and IP₃R-3 proteins, but lowered IP₃R-1 and IP₃R-2. All these changes are primarily related to elevated cytosolic Ca²⁺ as a consequence of changed composition of PMCAs. Interestingly, some of them could occur as adaptive processes protecting cells against calcium overload. Since age-related PMCA decrease has been documented [17, 45–47], our modified PC12 cells may be a useful model to clarify the biological changes in neurons associated with aging and, potentially, to study the vulnerability of cells to neurodegenerative insults.

The presence of CCR5 in PC12 cells was shown in several studies [25, 41], and it was also confirmed by our data. Moreover, we detected CCR1 and CCR3 proteins, but their cytosolic localization suggested that CCL5 signal was mainly transmitted by CCR5, because the activity of receptor requires its presence in the plasma membrane. Upregulation of CCR5 has been revealed in a number of neurological disorders and models of CNS injury, where it is often localized in astrocytes and microglial cells [48–51]. Overactivation of CCR5 with subsequent raise of cytosolic Ca²⁺ affected chemotaxis, secretion, and gene expression and could lead to inflammatory and degenerative processes in the CNS [27, 29]. Chemokine receptors could bind several chemokines and could act as multimeric forms, homo- or heterodimers [52–55]. The additional mechanism that may modify CCL5 signaling depends on the function of another type of calcium channels existing in ER, ryanodine receptors. RyRs are activated by a mechanism known as Ca²⁺-induced Ca²⁺ release (CICR) and involve cooperation with plasma membrane calcium channels [56]. Crucial for RyRs function is a high, micromolar Ca²⁺ concentration necessary to open these channels [57]. In our study, to avoid the potential influence of RyR-mediated secondary effects, we assayed CCL5 action without external calcium.

Using the selected inhibitors we confirmed that in our cell models CCL5 downstream effects involved CCR5-PLC-IP₃R pathway. The crucial step appeared to be associated with activation of IP₃ receptors. Although IP₃R-1 represents a predominant isoform in the central nervous system, other isoforms also exist in some brain areas and may differ in neuronal compartmentalization [58–60]. A particular role of IP₃Rs in hippocampus is related to learning and memory abilities, and changes in IP₃R isoforms composition during aging may have an impact on increased deficits in these processes. In most cultured cell types IP₃R-3 is the principal form, but IP₃R-1 and IP₃R-2 have also been detected [61]. All isoforms exhibit specific characteristics: IP₃R-1 possesses low Ca²⁺ affinity and medium affinity for IP₃, IP₃R-2 represents the isoform with the highest affinity for both Ca²⁺ and IP₃, and IP₃R-3 is the most sensitive for modulation by Ca²⁺, but displays the lowest IP₃ affinity [60]. Interestingly, IP₃Rs are regulated in a biphasic way by cytosolic Ca²⁺ and are stimulated at low Ca²⁺ level, but inhibited by higher than 300 nM Ca²⁺ [33]. Up to now, over 100 proteins have been identified to interact with and regulate the IP₃Rs [62]. Thus, multiple regulatory processes for each IP₃R isoform may produce diversified cell signaling paths that can initiate the adaptive response or can lead to neurodegeneration [60, 61].

Our analysis showed that in PC12 cells, all three IP₃R isoforms were present, with IP₃R-3 being the most prominent subtype. An interesting observation made here was the altered composition of IP₃Rs in PMCA-reduced lines at both mRNA and protein level. IP₃R-1 and IP₃R-2 decreased, whereas IP₃R-3 amount was higher than that of control cells. Changes in relative mRNA level indicate that the regulation occurs at the level of transcription, suggesting Ca²⁺-dependent negative feedback loop for IP₃R-1 and IP₃R-2. Analysis of IP₃R protein levels also confirmed the differences in a ratio of IP₃R isoforms between control _2 and _3 lines. One can assume that in both PMCA-reduced cells the decreased expression of receptors with higher affinity for IP₃ could lower the total apparent sensitivity to IP₃ and thereby may provide some protection against calcium overload. The graphical summary of these findings is presented in Figure 8.

Figure 8

Schematic presentation of CCL5 effect on PC12 cells. Downregulation of neurospecific PMCA2 or PMCA3 isoforms in differentiated PC12 cells generated two types of cell response: similar for both lines or characteristic for only one line. The common changes were increased cytosolic Ca²⁺ and, as a compensatory mechanism, upregulation of PMCA1 isoform, enlarged expression of SERCA2 and SERCA3, and diminished calmodulin amount [36, 40]. The levels of CCR5 and IP₃R-3 proteins also increased, but the expression of IP₃R-1 and IP₃R-2 was lowered (present study). Interestingly, altered IP₃R isoform composition did not change total IP₃R protein in the _2 line, while it increased in the _3 line. Also in _3 cells, the amount of PMCA4 increased [36]. These subtle differences could have profound consequences after CCL5/CCR5 activation, since potency to restore the basal Ca²⁺ level in the _3 line appears to be higher than in the _2 line, which may be essential for the survival of the cell. Under prolonged Ca²⁺ signal in the _2 line due to reduction of the fastest isoform - PMCA2, the subsequent Ca²⁺-mediated processes could increase vulnerability to cell death. Abbreviations used: CaM, calmodulin; CCL5, chemokine C-C motif ligand 5; CCR5, receptor for CCL5; inositol 1,4,5-triphosphate (IP₃); IP₃R, IP₃ receptor; PMCA, plasma membrane Ca²⁺-ATPase; SERCA, sarco/endoplasmic Ca²⁺-ATPase.

In _2 line, we observed higher Ca²⁺ accumulation in the ER; thus potentially more calcium could be released after activation of IP₃Rs. Moreover, less efficient PMCA-dependent extrusion system, due to PMCA2 suppression, may prolong calcium signaling, modifying a number of existing pathways. It can also lead to further Ca²⁺ overload. In fact, in this line we reported decreased cell survival and increased percentage of apoptotic cells [36]; thus the cells may exhibit higher vulnerability to calcium-induced cytotoxicity. Correlation between PMCA2 and disturbances in cell function resulting in augmented cell death has been reported in neurons, indicating a protective PMCA2 role [13, 63]. Taking into account the fact that PMCA2 represents nearly 40% of the total pump in the brain [64], reduction of PMCA2 appears to be more harmful for the cells than deficiency of PMCA3, and compensatory mechanisms may not be sufficient for full protection of cells.

The presence of an additional protective mechanism may be suggested in the _3 line, where we previously observed increased expression of PMCA4 isoform. One of the well-established mechanisms of PMCA regulation is stimulatory action of PIP₂ [9, 65, 66]. Recently, a new look on PMCA/PIP₂ interaction has been proposed [67]. Binding of PIP₂ by PMCA4 has been demonstrated to protect plasma membrane PIP₂ from hydrolysis by PLC. It could potentially limit IP₃ production and, subsequently, restrict Ca²⁺ release from ER. Since for full activity, IP₃Rs must bind four IP₃ molecules [68], a sufficient available PIP₂ concentration as a substrate for PLC is a necessary requirement. Accordingly, in the _3 line greater protection could result not only from the altered profile of IP₃Rs and the presence of highly active PMCA2, but also from higher PMCA4 amount. All these adaptive changes may limit the amount of Ca²⁺ released from the ER and shorten the time necessary to restore basal Ca²⁺ level.

5. Conclusions

Downregulation of neuron-specific PMCA2 or PMCA3 initiated a set of responses that significantly altered Ca²⁺-induced signaling that may allow cells to survive but also may promote cell death. The unique role played by “fast” isoforms of plasma membrane calcium pump in neuronal cells suggests that long-lasting calcium dyshomeostasis could markedly increase cell vulnerability to pathological events, including neurodegenerative disorders [13, 19, 63]. Aberration in the activity of PMCA2 has been implicated in some diseases, i.e., Huntington’s disease and multiple sclerosis, but altered expression of PMCA3 has been linked with cerebellar ataxia [69]. Here we demonstrated that CCL5/CCR5 signaling could be one of the critical mediators of the cell fate. Although we analyzed only the initial step in CCL5-induced pathway, this key phase could play a decisive role for the cell. In the aging brain increased BBB permeability, augmented leukocyte infiltration, and more severe CCL5 action under less efficient neuronal Ca²⁺ extrusion mechanism could accumulate potentially harmful changes in neurons, which increase the risk of developing neurodegenerative diseases.

Data Availability

All of data used to support the findings of this study are included within the article.

Conflicts of Interest

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as potential conflicts of interest.

Authors’ Contributions

Tomasz Radzik, Tomasz Boczek, Maciej Studzian, Lukasz Pulaski, and Ludmila Zylinska participated in research design and wrote, or contributed to the writing of, the manuscript; Tomasz Radzik, Bozena Ferenc, Maciej Studzian, and Lukasz Pulaski conducted the experiments; Tomasz Radzik, Tomasz Boczek, Maciej Studzian, Lukasz Pulaski, and Ludmila Zylinska performed data analysis.

Acknowledgments

This work was supported by grants nos. 503/6-086-02/503-61-001 and 502-03/6-086-02/502-64-086 from Medical University of Lodz, Poland. Tomasz Boczek is supported by “Mobility Plus” grant funded by the Polish Ministry of Science and Higher Education.

References

L. Cartier, O. Hartley, M. Dubois-Dauphin, and K.-H. Krause, “Chemokine receptors in the central nervous system: role in brain inflammation and neurodegenerative diseases,” Brain Research Reviews, vol. 48, no. 1, pp. 16–42, 2005.
View at: Publisher Site | Google Scholar
J. Chen, R. Mo, P. A. Lescure et al., “Aging is associated with increased T-cell chemokine expression in C57Bl/6 mice,” The Journals of Gerontology. Series A, Biological Sciences and Medical Sciences, vol. 58, no. 11, pp. B975–B983, 2003.
View at: Publisher Site | Google Scholar
A. Chou, K. Krukowski, J. M. Morganti, L.-K. Riparip, and S. Rosi, “Persistent infiltration and impaired response of peripherally-derived monocytes after traumatic brain injury in the aged brain,” International Journal of Molecular Sciences, vol. 19, no. 6, 2018.
View at: Google Scholar
H. N. Frazier, S. Maimaiti, K. L. Anderson et al., “Calcium's role as nuanced modulator of cellular physiology in the brain,” Biochemical and Biophysical Research Communications, vol. 483, no. 4, pp. 981–987, 2017.
View at: Publisher Site | Google Scholar
S. Orrenius, B. Zhivotovsky, and P. Nicotera, “Regulation of cell death: the calcium-apoptosis link,” Nature Reviews Molecular Cell Biology, vol. 4, no. 7, pp. 552–565, 2003.
View at: Publisher Site | Google Scholar
E. Pchitskaya, E. Popugaeva, and I. Bezprozvanny, “Calcium signaling and molecular mechanisms underlying neurodegenerative diseases,” Cell Calcium, vol. 70, pp. 87–94, 2018.
View at: Google Scholar
D. M. Sama and C. M. Norris, “Calcium dysregulation and neuroinflammation: Discrete and integrated mechanisms for age-related synaptic dysfunction,” Ageing Research Reviews, vol. 12, no. 4, pp. 982–995, 2013.
View at: Publisher Site | Google Scholar
E. Carafoli, “Calcium pump of the plasma membrane,” Physiological Reviews, vol. 71, no. 1, pp. 129–153, 1991.
View at: Publisher Site | Google Scholar
R. Lopreiato, M. Giacomello, and E. Carafoli, “The plasma membrane calcium pump: new ways to look at an old enzyme,” The Journal of Biological Chemistry, vol. 289, no. 15, pp. 10261–10268, 2014.
View at: Publisher Site | Google Scholar
E. E. Strehler, “Plasma membrane calcium ATPases: From generic Ca2+ sump pumps to versatile systems for fine-tuning cellular Ca2+,” Biochemical and Biophysical Research Communications, vol. 460, no. 1, pp. 26–33, 2015.
View at: Publisher Site | Google Scholar
E. E. Strehler and D. A. Zacharias, “Role of alternative splicing in generating isoform diversity among plasma membrane calcium pumps,” Physiological Reviews, vol. 81, no. 1, pp. 21–50, 2001.
View at: Publisher Site | Google Scholar
A. Kumar, J. R. Gibbs, A. Beilina et al., “Age-associated changes in gene expression in human brain and isolated neurons,” Neurobiology of Aging, vol. 34, no. 4, pp. 1199–1209, 2013.
View at: Publisher Site | Google Scholar
M. P. Kurnellas, H. Li, M. R. Jain et al., “Reduced expression of plasma membrane calcium ATPase 2 and collapsin response mediator protein 1 promotes death of spinal cord neurons,” Cell Death & Differentiation, vol. 17, no. 9, pp. 1501–1510, 2010.
View at: Publisher Site | Google Scholar
K. Pászty, A. K. Verma, R. Padányi, A. G. Filoteo, J. T. Penniston, and Á. Enyedi, “Plasma membrane Ca²⁺ATPase isoform 4b is cleaved and activated by caspase-3 during the early phase of apoptosis,” The Journal of Biological Chemistry, vol. 277, no. 9, pp. 6822–6829, 2002.
View at: Publisher Site | Google Scholar
E. E. Strehler and S. A. Thayer, “Evidence for a role of plasma membrane calcium pumps in neurodegenerative disease: recent developments,” Neuroscience Letters, vol. 663, pp. 39–47, 2018.
View at: Publisher Site | Google Scholar
B. L. Schwab, D. Guerini, C. Didszun et al., “Cleavage of plasma membrane calcium pumps by caspases: a link between apoptosis and necrosis,” Cell Death & Differentiation, vol. 9, no. 8, pp. 818–831, 2002.
View at: Publisher Site | Google Scholar
A. Zaidi, J. Gao, T. C. Squier, and M. L. Michaelis, “Age-related decrease in brain synaptic membrane Ca2+-ATPase in F344/BNF1 rats,” Neurobiology of Aging, vol. 19, no. 5, pp. 487–495, 1998.
View at: Publisher Site | Google Scholar
M. Berrocal, I. Corbacho, M. Vázquez-Hernández, J. Ávila, M. R. Sepúlveda, and A. M. Mata, “Inhibition of PMCA activity by tau as a function of aging and Alzheimer's neuropathology,” Biochimica et Biophysica Acta (BBA) - Molecular Basis of Disease, vol. 1852, no. 7, pp. 1465–1476, 2015.
View at: Publisher Site | Google Scholar
M. Brini, E. Carafoli, and T. Calì, “The plasma membrane calcium pumps: focus on the role in (neuro)pathology,” Biochemical and Biophysical Research Communications, vol. 483, no. 4, pp. 1116–1124, 2017.
View at: Publisher Site | Google Scholar
P. Hajieva, M. W. Baeken, and B. Moosmann, “The role of Plasma Membrane Calcium ATPases (PMCAs) in neurodegenerative disorders,” Neuroscience Letters, vol. 663, pp. 29–38, 2018.
View at: Publisher Site | Google Scholar
V. Khariv and S. Elkabes, “Contribution of Plasma Membrane Calcium ATPases to neuronal maladaptive responses: Focus on spinal nociceptive mechanisms and neurodegeneration,” Neuroscience Letters, vol. 663, pp. 60–65, 2018.
View at: Publisher Site | Google Scholar
G. Zanni, T. Cali, V. M. Kalscheuer et al., “Mutation of plasma membrane Ca2+ ATPase isoform 3 in a family with X-linked congenital cerebellar ataxia impairs Ca2+ homeostasis,” Proceedings of the National Acadamy of Sciences of the United States of America, vol. 109, no. 36, pp. 14514–14519, 2012.
View at: Publisher Site | Google Scholar
M. R. Pranzatelli, “Advances in biomarker-guided therapy for pediatric- and adult-onset neuroinflammatory disorders: targeting chemokines/cytokines,” Frontiers in Immunology, vol. 9, p. 557, 2018.
View at: Google Scholar
L. A. Campbell, V. Avdoshina, S. Rozzi, and I. Mocchetti, “CCL5 and cytokine expression in the rat brain: differential modulation by chronic morphine and morphine withdrawal,” Brain, Behavior, and Immunity, vol. 34, pp. 130–140, 2013.
View at: Publisher Site | Google Scholar
M. H. Park, Y. K. Lee, Y. H. Lee et al., “Chemokines released from astrocytes promote chemokine receptor 5-mediated neuronal cell differentiation,” Experimental Cell Research, vol. 315, no. 16, pp. 2715–2726, 2009.
View at: Publisher Site | Google Scholar
M. F. Lanfranco, I. Mocchetti, M. P. Burns, and S. Villapol, “Glial- and neuronal-specific expression of CCL5 mRNA in the rat brain,” Frontiers in Neuroanatomy, vol. 11, p. 137, 2018.
View at: Google Scholar
C. R. Balistreri, C. Caruso, M. P. Grimaldi et al., “CCR5 receptor biologic and genetic implications in age-related diseases,” Annals of the New York Academy of Sciences, vol. 1100, pp. 162–172, 2007.
View at: Publisher Site | Google Scholar
K. Gamo, S. Kiryu-Seo, H. Konishi et al., “G-protein-coupled receptor screen reveals a role for chemokine receptor CCR5 in suppressing microglial neurotoxicity,” The Journal of Neuroscience, vol. 28, no. 46, pp. 11980–11988, 2008.
View at: Publisher Site | Google Scholar
J.-P. Louboutin and D. S. Strayer, “Relationship between the chemokine receptor CCR5 and microglia in neurological disorders: consequences of targeting CCR5 on neuroinflammation, neuronal death and regeneration in a model of epilepsy,” CNS & Neurological Disorders: Drug Targets, vol. 12, no. 6, pp. 815–829, 2013.
View at: Publisher Site | Google Scholar
Y. Takeshita and R. M. Ransohoff, “Inflammatory cell trafficking across the blood-brain barrier: Chemokine regulation and in vitro models,” Immunological Reviews, vol. 248, no. 1, pp. 228–239, 2012.
View at: Publisher Site | Google Scholar
G. C. Wang and V. Casolaro, “Immunologic changes in frail older adults,” Translational Medicine @ UniSa, vol. 9, pp. 1–6, 2014.
View at: Google Scholar
R. E. Marques, R. Guabiraba, R. C. Russo, and M. M. Teixeira, “Targeting CCL5 in inflammation,” Expert Opinion on Therapeutic Targets, vol. 17, no. 12, pp. 1439–1460, 2013.
View at: Publisher Site | Google Scholar
M. J. Berridge, “The inositol trisphosphate/calcium signaling pathway in health and disease,” Physiological Reviews, vol. 96, no. 4, pp. 1261–1296, 2016.
View at: Publisher Site | Google Scholar
M. Iwai, T. Michikawa, I. Bosanac, M. Ikura, and K. Mikoshiba, “Molecular basis of the isoform-specific ligand-binding affinity of inositol 1,4,5-trisphosphate receptors,” The Journal of Biological Chemistry, vol. 282, no. 17, pp. 12755–12764, 2007.
View at: Publisher Site | Google Scholar
J. B. Parys and H. De Smedt, “Inositol 1,4,5-trisphosphate and its receptors,” Advances in Experimental Medicine and Biology, vol. 740, pp. 255–279, 2012.
View at: Google Scholar
T. Boczek, M. Lisek, A. Kowalski et al., “Downregulation of PMCA2 or PMCA3 reorganizes Ca²⁺ handling systems in differentiating PC12 cells,” Cell Calcium, vol. 52, no. 6, pp. 433–444, 2012.
View at: Publisher Site | Google Scholar
T. Boczek, M. Lisek, B. Ferenc et al., “Plasma membrane Ca²⁺-ATPase isoforms composition regulates cellular pH homeostasis in differentiating PC12 cells in a manner dependent on cytosolic Ca²⁺ elevations,” PLoS ONE, vol. 9, no. 7, Article ID e102352, 2014.
View at: Publisher Site | Google Scholar
T. Boczek, M. Lisek, B. Ferenc et al., “Silencing of Plasma Membrane Ca²⁺-ATPase Isoforms 2 and 3 Impairs Energy Metabolism in Differentiating PC12 Cells,” BioMed Research International, vol. 2014, Article ID 735106, 13 pages, 2014.
View at: Publisher Site | Google Scholar
T. Boczek, B. Ferenc, M. Lisek, and L. Zylinska, “Regulation of GAP43/calmodulin complex formation via calcineurin-dependent mechanism in differentiated PC12 cells with altered PMCA isoforms composition,” Molecular and Cellular Biochemistry, vol. 407, no. 1-2, pp. 251–262, 2015.
View at: Publisher Site | Google Scholar
T. Boczek, M. Lisek, B. Ferenc, and L. Zylinska, “Cross talk among PMCA, calcineurin and NFAT transcription factors in control of calmodulin gene expression in differentiating PC12 cells,” Biochimica et Biophysica Acta - Gene Regulatory Mechanisms, vol. 1860, no. 4, pp. 502–515, 2017.
View at: Publisher Site | Google Scholar
H. Tokami, T. Ago, H. Sugimori et al., “RANTES has a potential to play a neuroprotective role in an autocrine/paracrine manner after ischemic stroke,” Brain Research, vol. 1517, pp. 122–132, 2013.
View at: Publisher Site | Google Scholar
E. R. Chemaly, L. Troncone, and D. Lebeche, “SERCA control of cell death and survival,” Cell Calcium, vol. 69, pp. 46–61, 2018.
View at: Publisher Site | Google Scholar
L. Wang, K. J. Alzayady, and D. I. Yule, “Proteolytic fragmentation of inositol 1,4,5-trisphosphate receptors: a novel mechanism regulating channel activity?” The Journal of Physiology, vol. 594, no. 11, pp. 2867–2876, 2016.
View at: Publisher Site | Google Scholar
S. Marchi, S. Patergnani, S. Missiroli et al., “Mitochondrial and endoplasmic reticulum calcium homeostasis and cell death,” Cell Calcium, vol. 69, pp. 62–72, 2018.
View at: Publisher Site | Google Scholar
L. Jiang, M. D. Bechtel, N. A. Galeva, T. D. Williams, E. K. Michaelis, and M. L. Michaelis, “Decreases in plasma membrane Ca2+-ATPase in brain synaptic membrane rafts from aged rats,” Journal of Neurochemistry, vol. 123, no. 5, pp. 689–699, 2012.
View at: Publisher Site | Google Scholar
A. M. Mata, “Plasma membrane Ca²⁺-ATPases in the nervous system during development and ageing,” World Journal of Biological Chemistry, vol. 1, no. 7, pp. 229–234, 2010.
View at: Publisher Site | Google Scholar
A. Zaidi, M. Adewale, L. McLean, and P. Ramlow, “The plasma membrane calcium pumps—the old and the new,” Neuroscience Letters, vol. 663, pp. 12–17, 2018.
View at: Publisher Site | Google Scholar
U. De Fanis, G. C. Wang, N. S. Fedarko, J. D. Walston, V. Casolaro, and S. X. Leng, “T-lymphocytes expressing CC chemokine receptor-5 are increased in frail older adults,” Journal of the American Geriatrics Society, vol. 56, no. 5, pp. 904–908, 2008.
View at: Publisher Site | Google Scholar
K. Grabert, T. Michoel, M. H. Karavolos et al., “Microglial brain regiona dependent diversity and selective regional sensitivities to aging,” Nature Neuroscience, vol. 19, no. 3, pp. 504–516, 2016.
View at: Publisher Site | Google Scholar
A. Salminen, J. Ojala, K. Kaarniranta, A. Haapasalo, M. Hiltunen, and H. A. Soininen, “Astrocytes in the aging brain express characteristics of senescence-associated secretory phenotype,” European Journal of Neuroscience, vol. 34, no. 1, pp. 3–11, 2011.
View at: Publisher Site | Google Scholar
R. L. Yung and M. O. Ruran, “Aging is associated with increased human T Cell CC chemokine receptor gene expression,” Journal of Interferon & Cytokine Research, vol. 23, no. 10, pp. 575–582, 2003.
View at: Publisher Site | Google Scholar
L. D. Bennett, J. M. Fox, and N. Signoret, “Mechanisms regulating chemokine receptor activity,” The Journal of Immunology, vol. 134, no. 3, pp. 246–256, 2011.
View at: Publisher Site | Google Scholar
C. E. Hughes and R. J. B. Nibbs, “A guide to chemokines and their receptors,” FEBS Journal, vol. 285, no. 16, pp. 2944–2971, 2018.
View at: Publisher Site | Google Scholar
M. Mellado, J. M. Rodríguez-Frade, A. J. Vila-Coro et al., “Chemokine receptor homo- or heterodimerization activates distinct signaling pathways,” EMBO Journal, vol. 20, no. 10, pp. 2497–2507, 2001.
View at: Publisher Site | Google Scholar
M. Stone, J. Hayward, C. Huang, Z. E. Huma, and J. Sanchez, “Mechanisms of regulation of the chemokine-receptor network,” International Journal of Molecular Sciences, vol. 18, no. 2, p. 342, 2017.
View at: Publisher Site | Google Scholar
G. Santulli, D. Lewis, A. des Georges, A. R. Marks, and J. Frank, “Ryanodine receptor structure and function in health and disease,” Subcellular Biochemistry, vol. 87, pp. 329–352, 2018.
View at: Google Scholar
G. Meissner, “The structural basis of ryanodine receptor ion channel function,” The Journal of General Physiology, vol. 149, no. 12, pp. 1065–1089, 2017.
View at: Publisher Site | Google Scholar
J. K. Foskett, C. White, K. Cheung, and D. D. Mak, “Inositol trisphosphate receptor Ca2+ release channels,” Physiological Reviews, vol. 87, no. 2, pp. 593–658, 2007.
View at: Publisher Site | Google Scholar
J.-P. Decuypere, G. Monaco, L. Missiaen et al., “IP₃ Receptors, Mitochondria, and Ca²⁺ Signaling: Implications for Aging,” Journal of Aging Research, vol. 2011, Article ID 920178, 20 pages, 2011.
View at: Publisher Site | Google Scholar
T. Vervloessem, D. I. Yule, G. Bultynck, and J. B. Parys, “The type 2 inositol 1,4,5-trisphosphate receptor, emerging functions for an intriguing Ca2+-release channel,” Biochimica et Biophysica Acta (BBA) - Molecular Cell Research, vol. 1853, no. 9, pp. 1992–2005, 2014.
View at: Google Scholar
H. Ivanova, T. Vervliet, L. Missiaen, J. B. Parys, H. De Smedt, and G. Bultynck, “Inositol 1,4,5-trisphosphate receptor-isoform diversity in cell death and survival,” Biochimica et Biophysica Acta (BBA) - Molecular Cell Research, vol. 1843, no. 10, pp. 2164–2183, 2014.
View at: Publisher Site | Google Scholar
D. L. Prole and C. W. Taylor, “Inositol 1,4,5-trisphosphate receptors and their protein partners as signalling hubs,” The Journal of Physiology, vol. 594, no. 11, pp. 2849–2866, 2016.
View at: Publisher Site | Google Scholar
R. M. Empson, P. R. Turner, R. Y. Nagaraja, P. W. Beesley, and T. Knöpfel, “Reduced expression of the Ca2+ transporter protein PMCA2 slows Ca2+ dynamics in mouse cerebellar Purkinje neurones and alters the precision of motor coordination,” The Journal of Physiology, vol. 588, no. 6, pp. 907–922, 2010.
View at: Publisher Site | Google Scholar
E. Carafoli and J. Krebs, Calcium Homeostasis, Springer Berlin Heidelberg, Berlin, Germany, 1st edition, 2000.
View at: Publisher Site
D. Choquette, G. Hakim, A. G. Filoteo, G. A. Plishker, J. R. Bostwick, and J. T. Penniston, “Regulation of plasma membrane Ca2+ ATPases by lipids of the phosphatidylinositol cycle,” Biochemical and Biophysical Research Communications, vol. 125, no. 3, pp. 908–915, 1984.
View at: Publisher Site | Google Scholar
L. Missiaen, L. Raeymaekers, F. Wuytack, M. Vrolix, H. De Smedt, and R. Casteels, “Phospholipid-protein interactions of the plasma-membrane Ca2+-transporting ATPase. Evidence for a tissue-dependent functional difference,” Biochemical Journal, vol. 263, no. 3, pp. 687–694, 1989.
View at: Publisher Site | Google Scholar
J. T. Penniston, R. Padányi, K. Pászty, K. Varga, L. Hegedűs, and A. Enyedi, “Apart from its known function, the plasma membrane Ca2+atpase can regulate Ca2+ signaling by controlling phosphatidylinositol 4,5-bisphosphate levels,” Journal of Cell Science, vol. 127, no. 1, pp. 72–84, 2014.
View at: Publisher Site | Google Scholar
K. J. Alzayady, L. Wang, R. Chandrasekhar, L. E. Wagner, F. Van Petegem, and D. I. Yule, “Defining the stoichiometry of inositol 1,4,5-trisphosphate binding required to initiate Ca2+ release,” Science Signaling, vol. 9, no. 422, p. ra35, 2016.
View at: Google Scholar
X. Wu, L. Weng, J. Zhang, X. Liu, and J. Huang, “The plasma membrane calcium ATPases in calcium signaling network,” Current Protein & Peptide Science, vol. 19, no. 8, pp. 813–822, 2018.
View at: Publisher Site | Google Scholar

Copyright

Copyright © 2019 Tomasz Radzik et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

PDF Download Citation

Download other formats

Order printed copies

Views

1005

Downloads

1293

Citations

BioMed Research International

Calcium Dyshomeostasis Alters CCL5 Signaling in Differentiated PC12 Cells

Abstract

1. Introduction

2. Materials and Methods

2.1. Cell Culture

2.2. Ca2+ Measurement

2.3. RNA Isolation and Real-Time PCR

2.4. Western Blotting

2.5. Confocal Imaging

2.6. Data Analysis

3. Results

3.1. CCRs Expression in PC12 Cell Lines

3.2. CCL5 Effect on Calcium Transients

3.3. Analysis of PLC/IP3R Pathway

3.4. Characteristics of IP3 Receptors in PC12 Cell Lines

4. Discussion

5. Conclusions

Data Availability

Conflicts of Interest

Authors’ Contributions

Acknowledgments

References

Copyright

2.2. Ca²⁺ Measurement

3.3. Analysis of PLC/IP₃R Pathway

3.4. Characteristics of IP₃ Receptors in PC12 Cell Lines