ER-luminal [Ca2+] regulation of InsP3 receptor gating mediated by an ER-luminal peripheral Ca2+-binding protein
Abstract
Modulating cytoplasmic Ca2+ concentration ([Ca2+]i) by endoplasmic reticulum (ER)-localized inositol 1,4,5-trisphosphate receptor (InsP3R) Ca2+-release channels is a universal signaling pathway that regulates numerous cell-physiological processes. Whereas much is known regarding regulation of InsP3R activity by cytoplasmic ligands and processes, its regulation by ER-luminal Ca2+ concentration ([Ca2+]ER) is poorly understood and controversial. We discovered that the InsP3R is regulated by a peripheral membrane-associated ER-luminal protein that strongly inhibits the channel in the presence of high, physiological [Ca2+]ER. The widely-expressed Ca2+-binding protein annexin A1 (ANXA1) is present in the nuclear envelope lumen and, through interaction with a luminal region of the channel, can modify high-[Ca2+]ER inhibition of InsP3R activity. Genetic knockdown of ANXA1 expression enhanced global and local elementary InsP3-mediated Ca2+ signaling events. Thus, [Ca2+]ER is a major regulator of InsP3R channel activity and InsP3R-mediated [Ca2+]i signaling in cells by controlling an interaction of the channel with a peripheral membrane-associated Ca2+-binding protein, likely ANXA1.
Introduction
Modulating cytoplasmic free Ca2+ concentration ([Ca2+]i) is a universal signaling pathway that regulates numerous cell-physiological processes (Berridge, 2016). Ubiquitous endoplasmic reticulum (ER)-localized inositol 1,4,5-trisphosphate (InsP3) receptor (InsP3R) Ca2+-release channels play a central role in this pathway (Foskett et al., 2007). InsP3 generated in response to extracellular stimuli binds to and activates InsP3R channels to release Ca2+ stored in the ER lumen, generating diverse local and global [Ca2+]i signals (Berridge, 2016). Whereas much is known regarding regulation of InsP3R channel gating by multiple processes, including binding of cytoplasmic ligands (Ca2+, InsP3 and ATP4–), post-translational modifications, interactions with proteins, clustering and differential localization (Berridge, 2016), the regulation of InsP3R channel activity by Ca2+ concentration in the ER lumen ([Ca2+]ER) is poorly understood and controversial (see (Caroppo et al., 2003; Yamasaki-Mann and Parker, 2011) and references therein). InsP3R activity influences [Ca2+]ER, which is critical for many processes, including regulation of bioenergetics, protein biogenesis and folding, and Ca2+ signaling (Corbett and Michalak, 2000). [Ca2+]ER dysregulation is associated with pathological conditions, including ER stress responses, diabetes, cardiac dysfunction, neurodegeneration, defective cell proliferation and cell death (Berridge, 2016). Mechanisms that link cellular processes with [Ca2+]ER, and the connections between [Ca2+]ER dysregulation and disease pathogenesis are ill-defined and poorly understood (Mekahli et al., 2011).
For a long time, regulation of InsP3R channel activity by [Ca2+]ER has primarily been examined by approaches that relied on changes in [Ca2+]i or [Ca2+]ER to infer channel activity (Caroppo et al., 2003; Yamasaki-Mann and Parker, 2011) and references therein), with no rigorous control of both [Ca2+]ER and [Ca2+]i simultaneously. It has therefore been difficult to differentiate feed-through effects in which Ca2+ flux through channel raises [Ca2+]i at the cytoplasmic Ca2+-binding sites to modulate channel activity from direct effects of [Ca2+]ER on the luminal aspect of the InsP3R. Patch-clamp electrophysiology allows rigorous, simultaneous control of [Ca2+] on both sides of the membrane, but intracellular ER membranes are not accessible to patch pipettes. To overcome this limitation, we made use of the fact that the ER membrane is continuous with the outer nuclear membrane (Dingwall and Laskey, 1992) and pioneered the use of nuclear patch-clamp electrophysiology on isolated nuclei (Mak et al., 2005). This enables the activities of single InsP3R channels to be recorded in their native ER membrane and luminal milieus. Different patch-clamp configurations have been used to study single InsP3R channels under rigorously controlled [Ca2+]ER and [Ca2+]i: including on-nucleus (on-nuc, cytoplasmic aspect of the channel faces into the pipette solution with the luminal milieu intact, Figure 1A), excised luminal-side-out (lum-out, cytoplasmic aspect of the channel faces into the pipette solution with the luminal aspect exposed to the bath solution, Figure 1B) and excised cytoplasmic-side-out (cyto-out, cytoplasmic aspect of the channel perfused by the bath solution with the luminal aspect facing the pipette solution, Figure 1C; Mak et al., 2013a; Mak et al., 2013b). Because of the relatively low selectivity of InsP3R channels for Ca2+ vs K+ (15.2 : 1 [Vais et al., 2010a]) and orders of magnitude higher [K+] (140 mM) than that of other ions in the physiological solutions used in our experiments (70 nM to ≤600 μM [Ca2+]free; 0 or 200 μM [Mg2+]free), the electrical currents through open InsP3R channels are overwhelmingly carried by K+ in all our patch-clamp electrophysiology experiments, enabling the kinetics of channel gating to be studied with both luminal and cytoplasmic [Ca2+] well-defined and controlled.
Using the nuclear patch-clamp approach in a previous study (Vais et al., 2012), we demonstrated that InsP3R channel activity can be modulated by [Ca2+]ER indirectly via feed-through effects of Ca2+ flux driven through an open channel by high [Ca2+]ER that raises the local [Ca2+]i in the channel vicinity to regulate its activity through its cytoplasmic activating and inhibitory Ca2+-binding sites (Figure 2A). That study demonstrated that these feed-through effects can be completely abrogated by sufficient Ca2+ chelation on the cytoplasmic side to buffer local [Ca2+]i at cytoplasmic Ca2+ binding sites of the InsP3R. In the presence of 5 mM 5,5’-diBromo BAPTA (a fast acting Ca2+ chelator) on the cytoplasmic side in the lum-out excised patch configuration (Figure 1B), the open probability Po of the InsP3R channel did not change discernably when the [Ca2+]ER was switched between 70 nM and 300 μM, no matter whether saturating 10 μM [InsP3] (Figure 2C in Vais et al., 2012) or sub-saturating 3 μM [InsP3] (Figure 7B in Vais et al., 2012) was present in the micropipette (2 μM [Ca2+]i was in the micropipette in all experiments described here). Thus, as long as [Ca2+]free on the cytoplasmic side was well buffered, switching [Ca2+]ER between 70 nM and 300 μM in lum-out excised membrane patches had no effect on channel activity. This definitively ruled out the possibility that InsP3R activity is modulated directly by an intrinsic Ca2+-regulatory site on the luminal side that is either part of the InsP3R or of a protein that constitutively interacts with the channel (Figure 2B).
Notably, however, in all previous studies of InsP3R channel gating, nuclei were isolated into a bath solution with low [Ca2+]free to simulate physiological resting [Ca2+]i (Mak and Foskett, 2015). Although sarco/endoplasmic reticulum Ca2+-ATPase (SERCA) is present in the nuclear envelope (Lanini et al., 1992), the bath solutions contained no MgATP to energize it. Thus, passive Ca2+ leaks equilibrated [Ca2+]free in the perinuclear space of the isolated nuclei (effectively [Ca2+]ER) with bath [Ca2+] at unphysiologically low levels. Accordingly, possible [Ca2+]ER regulation of channel activity by peripheral proteins in the lumen that interact with the InsP3R only in the presence of high, physiological [Ca2+]ER (Figure 2C) would have been undetected in previous studies.
Here we specifically assessed whether such a peripheral luminal protein (PLP)-mediated [Ca2+]ER regulation of InsP3R channel activity exists. We discovered a strong Ca2+ flux-independent inhibition of InsP3R channel activity mediated by accessory ER-luminal protein(s) only in the presence of high, physiological [Ca2+]ER. We identified the region of the InsP3R that is involved in this [Ca2+]ER-dependent inhibition, and discovered that the widely expressed Ca2+-binding protein annexin A1 (ANXA1) localizes not only to the cytoplasm but also to the perinuclear space inside the nuclear envelope, and possibly in the ER lumen as well, where it plays a critical role in channel inhibition through high [Ca2+]ER-mediated interaction with the InsP3R. Reducing this interaction enhanced agonist-induced InsP3R-mediated Ca2+ release, and increased local elementary Ca2+-release events in intact cells. Thus, [Ca2+]ER is a major regulator of InsP3R-channel activity and InsP3R-mediated [Ca2+]i signaling in cells by controlling an interaction of the channel with a luminal peripheral membrane-associated Ca2+-binding protein, likely ANXA1.
Results
Novel regulation by [Ca2+]ER of InsP3R single-channel activity
We performed single-channel patch-clamp electrophysiology on outer membranes of nuclei isolated from mutant chicken B cells in which all three endogenous InsP3R genes were ablated and stably replaced with wild-type rat type-3 InsP3R (DT40-r3 cells) (Mak et al., 2005), so that homotetrameric rat type-3 InsP3R channels (Vais et al., 2012) were recorded in our experiments. In on-nuc patch-clamp experiments with the bath containing no MgATP, the [Ca2+]ER in the perinuclear space (Figure 3A) equilibrated with [Ca2+]bath (70 nM). Linear, ohmic InsP3R-channel current vs. applied potential (ich-Vapp) curves were observed with high single-channel conductance, as expected (Figure 3B). In contrast, with 1 mM MgATP in the bath solution (Figure 3C), SERCA activity raised [Ca2+]ER to physiological levels, if the outer and inner membranes of the isolated nuclei remained intact. The ich-Vapp curves (Figure 3D) observed were non-ohmic and asymmetric with respect to the origin, and single-channel conductance was reduced, both caused by permeant-ion (Ca2+) block of the measured K+ current due to high [Ca2+]ER. Thus, absence or presence of MgATP in the bath provides a mechanism to alter [Ca2+]ER in intact nuclei. In a previous study examining the Ca2+ permeant-ion effect on K+ conductance through InsP3R channels (Vais et al., 2010a), we derived an empirical equation that describes, with high accuracy, the InsP3R channel slope conductance over a broad range of [Ca2+]ER (0 to 1.1 mM). This enabled us to use the single-channel conductance, rather than Ca2+ indicator dye fluorescence, to estimate that [Ca2+]ER is ~300 μM in the perinuclear space of intact isolated DT40-r3 nuclei in the presence of bath MgATP. Subsequent excision of the membrane patch into the lum-out patch configuration (Mak et al., 2013c) exposed its luminal side to 70 nM [Ca2+]bath (Figure 3E), which restored linear Ich-Vapp curves and high single-channel conductance (Figure 3F).
In on-nuc patches of DT40-r3 nuclei, InsP3R channel open probability (Po) was high with 70 nM Ca2+ER (Figure 3H and L, red) whereas it was profoundly reduced with [Ca2+]ER raised to 300 μM by addition of MgATP to the bath (Figure 3H and L, blue). Even in saturating (10 μM) [InsP3], 300 μM Ca2+ER strongly reduced Po (Figure 3I and M, blue), to a level indistinguishable from that observed in 3 μM InsP3 (Figure 3L, blue). In contrast, when [Ca2+]ER = 70 nM, Po was higher in 10 μM InsP3 (Figure 3M, red) than in 3 μM InsP3 (Figure 3L, red). With the bath solution containing 1 mM MgATP and the SERCA inhibitor thapsigargin (2.5 μM) (Figure 3M, purple and Figure 3—figure supplement 1), Po was indistinguishable from that in 0-MgATPbath, confirming that bath MgATP raised [Ca2+]ER in intact nuclei by supporting SERCA activity. Because high concentrations of Ca2+ chelator (5 mM diBrBAPTA) buffered [Ca2+]i at cytoplasmic Ca2+ regulatory sites, possible feed-through effects were eliminated (Vais et al., 2012). Thus, with an intact ER-luminal milieu and [Ca2+]ER at a level characteristic of replete ER stores, InsP3R activity is profoundly suppressed by a mechanism unrelated to but as powerful as the well-known high-[Ca2+]i inhibition of InsP3R activity. Because luminal [Ca2+] does not directly affect InsP3R channel activity (Vais et al., 2012), these results suggest a novel regulatory mechanism, possibly mediated by a resident luminal Ca2+-binding protein.
After recording channel activity in the on-nuc patch-clamp configuration, patches were excised into the lum-out configuration to observe gating of channels with their luminal sides exposed to bath [Ca2+]free = 70 nM. Since [Ca2+]i and [Ca2+]ER experienced by channels in this configuration were effectively the same as those in the on-nuc configuration with no bath MgATP, it was expected that the inhibitory luminal-protein-mediated effect would be abrogated. In agreement, similar Po were observed for channels in this lum-out configuration (Figure 3J and M, green) and channels in the on-nuc configuration in 0-MgATP (Figure 3I and M, red). Importantly, channel Po remained high during subsequent perfusion with 300 μM Ca2+free (Figure 3K and M, brown). Lack of inhibition when [Ca2+] was raised to 300 μM suggests that the luminal effector mediating high-[Ca2+]ER inhibition is only loosely associated with the InsP3R, becoming irretrievably lost when the luminal side of the isolated patch was perfused by low-[Ca2+]free solution.
Since the levels of suppression of InsP3R channel activities in the presence of high [Ca2+]ER were independent of [InsP3] used (Figure 3L and M), all subsequent experiments were performed with saturating 10 μM [InsP3] to avoid possible ambiguous results due to insufficient stimulation of InsP3R channels.
To determine whether peripheral luminal-protein (PLP) inhibition affects endogenous InsP3R in different cell types, similar on-nuc patch-clamp experiments were conducted with intact nuclei (verified by asymmetric ich-Vapp curves [Figure 4A–C] and reduced single-channel conductance [Figure 4D–F]) isolated from mouse N2a cells, which predominantly express type 1 InsP3R (InsP3R–1) (Wojcikiewicz, 1995), rat PC-12 cells expressing mainly InsP3R-1 and InsP3R-3 (Newton et al., 1994), and wild-type (WT) chicken DT40 cells, which express all three isoforms (Sugawara et al., 1997). In a bath containing 0-MgATP, channels from the different cell types exhibited different maximum Po (Figure 4D–F red traces, and Figure 4G). With high [Ca2+]ER generated by 1 mM bath MgATP, Po of the various endogenous InsP3R channels were strongly suppressed (Figure 4D–F blue traces, and Figure 4H). Interestingly, Po of the different InsP3Rs were strongly suppressed to very similar extents (Po reduction: WT DT40 92%, PC-12 86%, N2a 90% (Figure 4I), comparable to that of InsP3R-3 in DT40-r3 cells (85%) (Figure 3M, red and blue). This suggests that the inhibitory protein is present in the ER lumen of many cell types and interacts with all three InsP3R isoforms under high [Ca2+]ER.
A luminal loop of the InsP3R is critical for luminal protein-mediated [Ca2+]ER regulation
We hypothesized that the PLP interacts directly with the InsP3R. Only a small fraction of the InsP3R sequence is exposed to the ER lumen, consisting of three loops (L1, L2, and L3) connecting transmembrane helices in the pore-forming domain. We selected human sequences (Figure 5A–C) based on structural information about the InsP3R (Fan et al., 2015). Since the inhibitory effects were observed in cells expressing different channel isoforms, we selected sequences conserved in all three InsP3R isoforms. We excluded the P-region (orange stripe) and selectivity filter (green stripe) involved in other crucial channel functions (Figure 5C). Only four short sequences (magenta stripes in Figure 5B–C) fit the criteria to be luminal region(s) of the InsP3R that could interact with the PLP.
We first investigated whether the conserved region of the L2 loop (pL2, Figure 5B) is involved, by recording InsP3R-3 channels in the cytoplasmic-side-out (cyto-out) configuration (Mak et al., 2013b) with pipette solutions that faced the luminal aspect of the channel containing synthetic pL2 peptides. Nuclei were first exposed to [Ca2+]bath = 70 nM and 0-MgATP, so [Ca2+]ER equilibrated with [Ca2+]bath at 70 nM (Figure 5D, left) promoting dissociation of PLP from the InsP3R. When the cyto-out patch configuration was achieved (Figure 5D, right), the luminal aspect of the channel faced the pipette solution containing [Ca2+]pip = 300 μM. Because the PLP had already dissociated from the channel before patch excision (Figure 5D, left), we expected no inhibition to be observed. Indeed, when the patch was perfused with saturating 10 μM InsP3 and optimal 2 μM Ca2+i (buffered with 5 mM dibromoBAPTA) (Vais et al., 2010b), channels were activated with reduced conductance due to permeant Ca2+ block caused by high [Ca2+]ER in the pipette solution, but they exhibited high Po (~0.6) (Figure 5G and J, magenta) indistinguishable from that observed in on-nuc experiments under similar conditions (red bars in Figure 5J). Alternately, nuclei were first exposed to 1 mM MgATP in the bath to raise [Ca2+]ER to ~300 μM to promote an interaction between the PLP and the InsP3R (Figure 5E, left). Because the pipette solution contained 300 μM Ca2+, the interaction remained intact when the cyto-out patch configuration was achieved (Figure 5E, right). Indeed, low channel Po was observed with maximal stimulation (Figure 5H and J, purple), similar to the observations made using the on-nuc configuration (Figure 5J, blue bars). Having therefore established that the inhibitory effect of the PLP could be observed in the cyto-out patch configuration, we included 10 μM pL2 peptide in the pipette solution (Figure 5F, left). With pL2 peptides present on the cytoplasmic side in the on-nuc configuration before establishing the cyto-out configuration, InsP3R remained bound to the PLP before membrane excision. However, after achieving the cyto-out configuration, the luminal side of the InsP3R became exposed to the peptides. We reasoned that if the pL2 region is involved in the inhibitory effects through interactions with the PLP, then pL2 peptide in high concentrations should compete the PLP away from the InsP3R, and thereby raise Po despite presence of 300 μM Ca2+ (Figure 5F, right). Indeed, inhibition was completely abolished such that the Po of channels with pL2 peptides on their luminal side (Figure 5I–J, brown) was indistinguishable from Po recorded in on-nuc (red) or cyto-out patch-clamp experiments with 0-MgATP in the bath (magenta). This indicates that the pL2 region interacts with the PLP to suppress InsP3R channel activity, and that the inhibitory effect of the PLP is mostly or completely mediated by the pL2-PLP interaction.
Identification of the inhibitory peripheral protein(s) in the ER lumen
To identify the PLP, peptides with a modified pL2 sequence (mpL2) or scrambled mpL2 (smpL2) were used for in-vitro pull-downs from soluble fractions of bovine hepatocyte ER microsomes (Figure 6—figure supplement 1). Eluates from the pull-downs were analyzed by mass spectrometry. Among >460 proteins detected, we looked for those enriched in the mpL2, that are Ca2+-binding proteins (UniProt protein database) in the ER lumen (or in topologically-equivalent locations), and that are broadly expressed. The annexin (ANX) protein family met these criteria. Of 12 members of the ANX family, five were identified to have statistically-significant preference to bind to the mpL2 peptide over the smpL2 peptide (Figure 6—source data 1, also see ‘Ca2+-dependent affinity enrichment mass spectrometry’ in Materials and methods).
ANX proteins are ubiquitously expressed, Ca2+-dependent phospholipid-binding proteins (Raynal and Pollard, 1994). Ca2+ binding to ANX (dissociation constant Kd ~25 μM to 1 mM) promotes its association with negatively-charged phospholipid-containing membranes (Raynal and Pollard, 1994; Gerke and Moss, 2002). Although ANX proteins are known to be cytoplasmic, many studies have reported their presence in locations topologically equivalent to the ER lumen, including the extracellular side of the plasma membrane (PM) (Solito et al., 1994; Brownstein et al., 2001; McArthur et al., 2009; Yáñez et al., 2012; Mirkowska et al., 2013), within intracellular and secretory granules (McArthur et al., 2009; Leoni et al., 2015; Chi et al., 2006; Boudhraa et al., 2016; Perretti et al., 2000), and in the extracellular space (McArthur et al., 2009; Boudhraa et al., 2016; Arur et al., 2003; Fan et al., 2004; Scannell et al., 2007; D'Acquisto et al., 2007; Iwasa et al., 2012; Belvedere et al., 2014), suggesting that ANX can also be present in the ER lumen.
Among annexins, ANXA1 is most widely reported to be present in locations topologically equivalent to the ER lumen. To confirm that ANXA1 was present in the ER lumen, we localized it by immunofluorescence microscopy. A549 cells were briefly exposed to a low concentration of digitonin to permeabilize the PM to release cytoplasmic ANXA1. Remaining ANXA1 co-localized with the ER marker calnexin in the nuclear envelope and in cytoplasmic puncta (Figure 6A). ANXA1 localization to the nuclear envelope was also observed in HeLa and Panc-1 cells (Figure 6B–D). The inability to observe ANXA1 throughout the ER could be the result of its low expression in the bulk ER lumen. Therefore, to further establish localization to the ER lumen, we performed capture ELISA of secreted proteins. The non-secreted β-actin was detected only in the lysate (Figure 6E, blue), indicating that the HEKtsA201 cells remained healthy and intact during the 3 day incubation period. In contrast, the signal for extracellular ANXA1 was robust (Figure 6E, red), suggesting that ANXA1 was present in the ER lumen en route to be secreted.
Luminal ANXA1 can mediate [Ca2+]ER-dependent InsP3R channel inhibition
We examined direct effects of ANXA1 on channel gating in cyto-out patch-clamp experiments with pipette solutions (bathing the luminal side) containing 1 μM recombinant full-length human ANXA1 under conditions that prevented permeant Ca2+ feed-through effects (Figure 7—figure supplement 1). ANXA1 was without effect on maximally-stimulated channel Po (≈ 0.65) in [Ca2+]ER between 70 nM and 55 μM (Figure 7A–C and F). In contrast, with [Ca2+]ER >55 μM, channel Po dropped abruptly with increasing [Ca2+]ER (Figure 7D–F). Fitting the Po data with a simple inhibitory Hill equation (Figure 7F):
showed that the half-maximal inhibitory [Ca2+]ER (Kinh) is 260 ± 14 μM with Hill coefficient (Hinh) of 2.3 ± 0.3 (Figure 7F). The observed Kinh is within observed physiological levels of [Ca2+]ER (~100 μM to 1 mM) (Zampese and Pizzo, 2012) and Kd of ANX binding to Ca2+. Without affecting the number of channels observed (Figure 7G), ANXA1 inhibited Po mainly by increasing channel-closed durations (Figure 7H–I).
ANXA1 is primarily localized to the cytoplasm. However, ANXA1 on the cytoplasmic side of the InsP3R was without affect (Figure 7J–L). Thus, ANXA1 inhibits InsP3R activity exclusively from the luminal side.
ANXA1 inhibits InsP3R channel gating by interacting with the L2 loop region
To determine if ANXA1 inhibition is mediated by interaction with the L2 loop, we performed cyto-out patch-clamp experiments with the pipette solution facing the luminal aspect containing 1 μM ANXA1 and 40 μM of peptides with either the L2 sequence or a scrambled L2 (sL2) sequence (Figure 8A–B, respectively) to compete with the InsP3R for binding to ANXA1 (Figures 5J and 7F). The L2 peptide, but not the sL2 peptide, completely abrogated inhibition of InsP3R activity by ANXA1 (Figure 8C). This suggests that suppression of channel activity by ANXA1 is specifically mediated by the L2 region of the InsP3R.
Native PLP-mediated and recombinant ANXA1-mediated [Ca2+]ER-dependent InsP3R channel inhibition have similar features
In sub-physiological 70 nM Ca2+ER, neither the native PLP (Figure 9, Lane 2) nor recombinant ANXA1 (Figure 9, Lane 5) suppressed channel activities, since Po observed were indistinguishable from those with no PLP on the luminal side (Figure 9, Lane 1). In 300 μM Ca2+ER, both native PLP (Figure 9, Lane 3) and luminal ANXA1 (Figure 9, Lane 6) inhibited the Po. Inhibition by PLP or ANXA1 was completely abrogated by L2 loop peptides (Figure 9, Lanes 4 and 7, respectively). Such similarities suggest that ANXA1 is the major PLP mediating [Ca2+]ER-dependent inhibition of InsP3R channels.
Although native PLP and luminal ANXA1 both inhibit InsP3R activity, Po of PLP-inhibited InsP3R channels (Figure 9, Lane 3) was lower than that of ANXA1-inhibited channels (Figure 9, Lanes 6 and 8). However, in higher [Ca2+]ER (600 μM), ANXA1-inhibited channel Po (Figure 9, Lane 9) was comparable to the native PLP-inhibited Po (Figure 9, Lane 3). This suggests that the luminal concentration of endogenous ANXA1 is effectively higher than 1 μM, and/or that other factor(s) enhance the [Ca2+]ER sensitivity of the channel to inhibition by ANXA1.
Annexin A1 specifically mediates [Ca2+]ER-dependent InsP3R channel inhibition
Multiple annexins were identified in our mass spectroscopy analysis, including ANXA6, ANXA2 and ANXA11 (Figure 6—source data 1). However, recombinant ANXA6 or ANXA2 had no effect on channel Po (Figure 10A–B). Similar experiments with ANXA11 were precluded by its low solubility. The ANXA6 used had an N-terminal His tag. However, suppression of InsP3R activities by ANXA1 with and without an N–terminal His tag was equivalent (Figure 10—figure supplement 1), indicating that the observed effects were not impacted by presence or absence of the tag.
Annexins have a conserved C-terminal ‘annexin core’ domain with multiple ‘annexin-type’ Ca2+-binding sites (Gerke and Moss, 2002). In contrast, the N-terminal regions are diverse (Raynal and Pollard, 1994). That ANXA1, but neither ANXA6 nor ANXA2, inhibited gating of InsP3R channels suggests that inhibition is mediated by interaction of its N-terminal domain with the InsP3R. To determine if the N-terminal domain itself can affect channel activity, we included 32 μM N-terminal peptide of human ANXA1 (Figure 10C) in the pipette solution with 300 μM Ca2+ER, and found that channel Po was unaffected (Figure 10D–E). This suggests that whereas the N-terminal domain may mediate interaction between ANXA1 and the InsP3R L2 region, the ANXA1 C-terminal domain is likely needed to localize ANXA1 to the two-dimensional surface of the ER membrane to increase its local concentration to facilitate N-terminus binding to the InsP3R to suppress channel activity.
Endogenous ANXA1 inhibits InsP3R-mediated Ca2+ release in intact cells
To determine effects of ANXA1 on cytoplasmic Ca2+ signaling, we used siRNA to reduce ANXA1 protein expression after 48 hr to ~35% of WT levels in HEKtsA201 cells (Figure 11A–B), and measured magnitude (ΔRmax) and rate of change (1/τ) of Fura-2 fluorescence ratio in populations of cells responding to the muscarinic receptor agonist carbachol (Figure 11C) in a bath solution containing 1.5 mM CaCl2. These parameters capture the initial InsP3R-mediated Ca2+-release phase of the response to agonist. Both parameters were enhanced specifically in the ANXA1 siRNA-treated cells (Figure 11D–E, respectively), suggesting that endogenous ANXA1 inhibits InsP3R-mediated Ca2+ release.
We also measured histamine-induced changes in Fura-2 fluorescence ratio (R/R0) in individual ANXA1 and non-targeting (N-T) siRNA-treated HeLa cells (Figure 11F). Saturating (100 µM) histamine elicited similar responses in both kinds of siRNA-treated cells (Figure 11H). In contrast, in sub-saturating (10 µM) histamine, an increase in both the fraction of responding cells (Figure 11G) and the maximal increase in R/R0 was observed in the ANXA1 siRNA-treated cells (Figure 11I). We classified responding cells as ‘oscillatory’ or ‘non-oscillatory’ (Figure 11K). In 100 µM histamine, the fraction of ocillatory cells was indistinguishble between AnxA1 or N-T siRNA-treated cells; whereas in 10 µM histamine, a significantly higher fraction of ANXA1 siRNA-treated cells showing either ‘random spiking’ or ‘periodic oscillations’ (Figure 11J).
We explored this further by visualizing elementary Ca2+-release events (Ca2+ puffs) generated by clusters of InsP3R stimulated by uncaging of a non-metabolizable InsP3 analogue (Figure 11L; Lock et al., 2018). More Ca2+ puffs were observed in the cells treated with ANXA1-siRNA than in cells treated with non-targeting siRNAs (Figure 11M–N), with larger amplitudes (Figure 11O–P), regardless of whether they were generated by a sub-saturating UV flash (50 ms, Figure 11M and O) or a saturating one (150 ms, Figure 11N and P). Taken together, these results suggest that endogenous luminal ANXA1 inhibits InsP3R-mediated Ca2+ release in vivo, in strong agreement with the strong inhibition by ANXA1 of InsP3R channel activity observed in vitro.
Discussion
A novel mechanism of strong regulation of InsP3R channel activity by ER [Ca2+]
Our study has established that physiological [Ca2+]ER in the normally-replete ER lumen strongly inhibits the activity of the InsP3R Ca2+-release channel, with consequent effects on InsP3-mediated Ca2+ signals in cells. This inhibitory effect is not mediated by direct Ca2+ binding to luminal sites on the InsP3R nor by flux-through effects of Ca2+ on cytoplasmic regulatory sites. Rather, it is mediated by a direct interaction of the InsP3R with a lumen-localized membrane-associated protein, which is likely to be ANXA1.
We first established that high [Ca2+]ER strongly inhibits InsP3R channel activity by a mechanism involving a putative ER-luminal peripheral protein. To identify the protein, we focused on a segment that is highly conserved in all three InsP3R isoforms and which, according to a 2015 cryo-EM structure (Fan et al., 2015), is located as a luminal loop (L2) between transmembrane helices TM3 and TM4 of InsP3R-1. Interestingly, the L2 sequence was assigned to a different location in a recent cryo-EM structure of InsP3R-3 (Paknejad and Hite, 2018). Nevertheless, we discovered ANXA1 by pull-down with the pL2 peptide, and inhibition of channel activity by high [Ca2+]ER was relieved by inclusion of L2 peptides in the ER lumen. These experiments establish that the inhibition of InsP3R activity is mediated through a protein interaction with the InsP3R L2 region. The structures in Paknejad and Hite, 2018 have closed channel pores despite binding of InsP3 and Ca2+. Of note, ANXA1 reduces, but does not completely abrogate activity of the InsP3R. It is possible that the topology of the L2 region is different in functionally distinct channel-activation states, with some states enabling it to interact in the ER lumen with ANXA1.
Whereas the predominance of our data suggests that the luminal protein responsible for InsP3R inhibition in high [Ca2+]ER is ANXA1, some results give us pause. First, we have been unable to co-immunoprecipitate (co-IP) the two proteins from cell lysates. There are many reasons why co-IP can fail, including low expression of ANXA1 in the ER lumen, particularly in comparison with its strong expression in the cytoplasm; and that the interacting regions in InsP3R and ANXA1 are small, particularly in the case of the InsP3R. Second, whereas we have been able to apply immunofluorescence microscopy to localize ANXA1 to the nuclear envelope in different permeabilized cells with cytoplasmic ANXA1 washed out, localization to the ER has been unconvincing (Figure 3A–E). This may reflect a very low abundance of luminal ANXA1 in the peripheral ER that escapes detection. Third, effects of ANX1A knockdown on intracellular Ca2+ signaling were modest (Figures 11D–E,G–J,M–P). This could be due to the fact that knockdown reduced the ANXA1 expression level by only about 65% (Figure 11B and F). Taken together, these results may suggest that ANXA1 is not the bona fide PLP. Other ER-luminal proteins have also been reported to regulate InsP3R activity, but their effects are all very different from those of the PLP defined here. Direct interaction with chromogranins enhances activity (Yoo and Lewis, 2000), and BiP/Grp78 promotes tetramerization of InsP3R-1, thereby enhancing Ca2+ release (Higo et al., 2010). In contrast, the PLP here inhibits InsP3R channel activity. Thioredoxin ERp44 interacts directly with InsP3R to suppress channel activity (Higo et al., 2005). However, ERp44-mediated inhibition is reduced as [Ca2+]ER increases beyond 100 μM, a [Ca2+]ER dependence opposite to that of the PLP defined here. Furthermore, ERp44 interacts specifically with InsP3R-1, whereas the PLP here inhibits all InsP3R isoforms.
Annexins are defined by a conserved C-terminal Ca2+ binding domain (Gerke and Moss, 2002). Although the intrinsic affinity of ‘annexin-type’ Ca2+ binding sites is low (Kd up to mM range) (Raynal and Pollard, 1994), the presence of phospholipids, especially those with negatively-charged headgroups, strongly enhances Ca2+ affinity (Gerke and Moss, 2002). Conversely, the affinity of annexins for acidic phospholipids increases dramatically in the presence of high [Ca2+]free (Raynal and Pollard, 1994; Gerke and Moss, 2002). This feature is likely the mechanism underlying the [Ca2+]ER dependence of ANXA1 inhibition of InsP3R activity. In low [Ca2+]ER, ANXA1, having low affinity for phospholipids, remains in the bulk ER lumen, rendering an interaction between ANXA1 and InsP3R channels that are confined to the ER membrane highly unfavorable entropically. With no ANXA1 interaction, the channel can gate robustly. In contrast, in high [Ca2+]ER (>100 μM, Figure 7F), the ANXA1 C-terminus binds to phospholipids with high affinity and become restricted to the surface of the ER membrane. This substantially increases the chances for ANXA1 to interact with the InsP3R, which promotes channel inhibition.
Physiological implications of ANXA1 regulation of the InsP3R
Inhibition of InsP3R by the PLP is very potent. With [Ca2+]ER sufficiently high (≥300 μM), the PLP and ANXA1 strongly suppressed channel activation even in optimal concentrations of cytoplasmic Ca2+ and InsP3, such that channel Po is limited to ~0.1 (Figure 7F), merely 15% of the maximal Po elicited by saturating [InsP3] in absence of PLP (ANXA1) (Vais et al., 2012). This powerful effect is comparable in magnitude to the maximal inhibition of InsP3R activity by high (50 μM) [Ca2+]i (Vais et al., 2012). Furthermore, the range of [Ca2+]ER over which this regulation occurs is within the physiological range. [Ca2+]ER in fully-replete stores has been measured to be 250 μM – 1 mM (Zampese and Pizzo, 2012). We observed strong channel inhibition at 300 μM, with more profound inhibition at 600 μM. During agonist stimulation, bulk [Ca2+]ER falls to concentrations that activate STIM1, which has an apparent luminal-Ca2+ affinity of 200–400 μM (Suzuki et al., 2014; Stathopulos et al., 2008). We observed apparent Ca2+ affinity of ANXA1-mediated inhibition of ~250 μM, suggesting that relief of inhibition will occur under physiological conditions that activate STIM1 and store-operated Ca2+ entry.
It has been suggested that most InsP3R channels (~95%) in cells are unresponsive to experimentally-induced elevations of [InsP3], with responsive channels limited to those in immobile clusters from which Ca2+ blips and puffs originate (Lock et al., 2019; Keebler and Taylor, 2017; Thillaiappan et al., 2017). The mechanisms that silence the majority of InsP3R are unknown, but our results indicate that the PLP defined here (ANXA1) could play a role. In this scenario, most InsP3R are normally associated with the PLP, rendering them unresponsive to InsP3. However, channels in some clusters may lose their association with the PLP, possibly because of a unique phospholipid composition of the ER membrane there, or because the L2 sequence is not exposed in InsP3R channels in clusters, or for other reasons. Channels in such clusters would be much more responsive to InsP3 and ‘licensed’ to respond even with the ER fully replete with Ca2+. In addition, the strong inhibition of InsP3R channel activity by ANXA1 could possibly help shape intracellular InsP3-induced Ca2+ signals. PLP (ANXA1) inhibition will reduce the amount of Ca2+ released by shortening the open durations of activated channels (Figure 7H) and reducing their frequency by lengthening their closed durations (Figure 7I). With fewer Ca2+ release events with reduced magnitude, coordination by released Ca2+ from channels in a cluster to generate Ca2+ puffs can be hampered, preventing puffs from being organized into global Ca2+ signals. Such suppression of Ca2+ release by the PLP could ensure spatial fidelity of local Ca2+ signals and be a fail-safe mechanism to prevent excessive, detrimental release of Ca2+ from the ER. At reduced [Ca2+]ER, the PLP regulation of InsP3R activity could also be a mechanism to preserve fidelity of Ca2+ signals. As [Ca2+]ER drops, the [Ca2+] gradient across the InsP3R is reduced, and the Ca2+ flux it drives through the pore decreases. Between 100 and 600 μM [Ca2+]ER, the six-fold reduction in Ca2+ flux could be compensated by the ~6.6 fold increase in the Po of the InsP3R channels (from ~0.09 to 0.6) as PLP inhibition of channel activity is alleviated (Figure 7F). This could allow the amount of Ca2+ released to be maintained despite the drop in [Ca2+]ER to preserve Ca2+ signals required to regulate downstream cellular processes.
Limitations of the current study
As noted, co-immunoprecipitation of ANXA1 with the InsP3R was not successful. Further studies, using different methods and antibodies should be performed to determine whether the proteins physically interact.
As noted, ANXA1 was secreted into the bath (Figure 6E), but its localization in permeabilized cells was evident only in the nuclear envelope (Figure 6A–D), and not in the peripheral ER. On the other hand, AnxA1 was initially identified as a potential protein that interacts with the InsP3R through in-vitro pull-down assays and mass spectrometry, using ultra-centrifuged ruptured ER microsome fraction devoid of nuclei. Additional studies employing different antibodies and imaging techniques, including super-resolution light microscopy and electron microscopy should be performed to establish the presence of ANXA1 in the lumen of the entire ER.
We demonstrated increased channel Po in the presence of the pL2 peptide and concluded that it was caused by the peptide reversal of the inhibition by luminal Ca2+. A control experiment to demonstrate that the pL2 peptide does not increase channel Po under conditions with reduced luminal [Ca2+] should be performed. We note however that the channel Po is already very high under conditions of reduced luminal [Ca2+]. In a control experiment, we could change the conditions, for example use lower [InsP3] to observe channels with a low channel Po in conditions of reduced luminal [Ca2+].
Materials and methods
Proteins
Recombinant full-length human annexin proteins from Abcam were used in our experiments: ANXA1 (cat. # ab86446 with no tag; ab184588 with N-terminal His tag), Anx A2 (cat. # ab93005 with N-terminal His tag), and Anx A6 (cat. # ab92934 with N-terminal His tag).
Synthetic peptides
Request a detailed protocolPeptides used in our study: L2 (GNRGTFIRGYKAMVMDMEFLYHVGYILTSVLGLFAHEL), sL2 (DVVIALHGNAMMYLLVFEHTSTGIGKFLRFYGERLMYG), pL2 (GNRGTFIRGYKAMVMDME), mpL2 (K-Ahx-GNRGTFIRGYRAMVMDME, Ahx stands for 6-aminohexanoate residue), smpL2 (K-Ahx-RDYRGMRMIMGETFNVGA), and ANXA1 N-terminal peptide (MAMVSEFLKQAWFIENEEQEYVQTVKSSKGGPGSAVSPYPT) were custom synthesized by Peptide 2.0 (Chantilly, VA).
Generation and maintenance of cell lines
Request a detailed protocolAll cell lines used were obtained from commercial sources and were routinely tested and confirmed to be mycoplasma-free via PCR. Wild-type DT40 chicken B cells and DT40-KO cells in which all three endogenous InsP3R genes have been stably ablated were obtained from Riken Bioresource Center, Japan (cell bank # RCB1464 and RCB1467, respectively). Generation of DT40–KO-r–InsP3R–3 cells (DT40-r3 cells) that stably express only recombinant rat type 3 InsP3R in DT40-KO cells was described in Mak et al., 2005. Wild type DT40 and DT40-r3 cells used in this study were grown in suspension culture in RPMI 1640 medium with 2 mM L-glutamine (Gibco cat. # 11875–085), supplemented with 10% (v/v) FBS, 1% chicken serum, and 1% Gibco antibiotic-antimycotic, and 1% G418 for selection; at 37°C in 5% CO2. When cell density exceeded 2.5 × 106/ml, they were sub-cultured to 0.1–0.2 × 106/ml (Mak et al., 2005).
Wild type HEK293 cells from ATCC (CRL-1573) and InsP3R-Null HEK-293 cells with all three endogenous InsP3R genes knocked out by CRISPR/Cas9 technology (HEK-3KO) from Kerafest (cat. # EUR030) were cultured as adherent cells in DMEM (with L-glutamine, glucose and sodium pyruvate; Corning cat. # MT10-013-CM), supplemented with 10% FBS and 1% Gibco antibiotic-antimycotic; at 37°C in 5% CO2. Medium was renewed every two to three days. Cells were sub-cultured following instructions provided in ATCC CRL-1573 product sheet.
HEK-3KO cells stably expressing rat InsP3R-3 (HEK–3KO-r–InsP3R–3) were generated from HEK293-3KO cells by transfecting them using Transit LT-1 (Mirus cat. # MIR 2304) following manufacturer’s protocols. Using G418 selection, stable clones of HEK293-3KO-r-InsP3R-3 cells expressing various level of recombinant r-InsP3R-3 were generated by limiting dilution.
Mouse N2a cells from ATCC (CCL-131) were cultured as adherent cells in 1:1 mixture of DMEM (high glucose with L-glutamine; Gibco cat. # 11965–092) and Opti-MEM I Reduced Serum Medium (Gibco cat. # 31985–070), supplemented with 5% FBS, 1% penicillin-streptomycin; at 37°C in 5% CO2. Cells were sub-cultured following instructions provided in ATCC CCL-131 product sheet.
Rat PC12 cells from ATCC (CRL-1721) were cultured as adherent cells in F-12K Kaighn’s Mod. Nutrient mixture (Corning Catalog # 10–025-CV), supplemented with 15% horse serum, 2.5% FBS, 1% Gibco antibiotic-antimycotic; at 37°C in 5% CO2. Cells were sub-cultured following instructions provided in ATCC CRL-1721 product sheet.
Human HEKtsA201 cells derived from HEK293 cells were obtained from Sigma-Aldrich (cat. # 96121229) and cultured as adherent cells in the same medium as for HEK293 cells, at 37°C in 5% CO2. 70–80% sub-confluent cells were dislodged using 0.25% trypsin solution and split 1:4 to 1:8 as described in ECACC data sheet for HEKtsA201 cells.
A549 human carcinoma cells from ATCC (CCL-185) were cultured using the same protocol as that for HEKtsA201 and HEK293 cells.
Panc-1 human pancreatic epithelioid carcinoma cells from ATCC (CRL-1469) were cultivated as adherent cells in DMEM with L-glutamine, glucose and sodium pyruvate (Corning cat. # MT10-013-CM), supplemented with 10% FBS and 1% Gibco antibiotic-antimycotic; at 37°C in 5% CO2. Cells were sub-cultured following instructions provided in ATCC CCL-1469 product sheet.
Nuclear patch-clamp electrophysiology
Request a detailed protocolIsolation of intact nuclei from cells, performing nuclear patch-clamp experiments in on-nucleus, cytoplasmic-side-out and luminal-side-out configurations with rapid exchange of ligand conditions are described in detail in Mak et al., 2013b; Mak et al., 2013c; Vais et al., 2010b. All solutions used for nuclear patch-clamp experiments contained 140 mM KCl, 10 mM HEPES (pH 7.3). Solutions on the cytoplasmic side of the nuclear membrane contained 2 μM free [Ca2+] ([Ca2+]free). [Ca2+]free was buffered either by 0.5 mM 5,5′-dibromo 1,2-bis(o-aminophenoxy)ethane-N,N,N′,N′-tetraacetic acid (diBrBAPTA, Invitrogen D-1211 or Santa Cruz Biotechnology sc-2273516) in experiments in which [Ca2+]free on the luminal side of the membrane ≤300 μM; or by 5 mM diBrBAPTA or 10 mM N-(2-Hydroxyethyl)ethylenediaminetriacetic acid (HEDTA, Sigma H7154) in experiments with luminal [Ca2+]free ≥300 μM to eliminate possible permeant Ca2+ feed-through effects on InsP3R channel activities (Vais et al., 2012). Cytoplasmic solutions also contained 0.5 mM Na2ATP (Mak et al., 2001) and either sub-saturating 3 μM or saturating 10 μM [InsP3] (Vais et al., 2012) (Invitrogen I-3716 or Santa Cruz Biotechnology sc-201521) to stimulate InsP3R channel gating. The luminal solution with 70 nM [Ca2+]free was buffered by 0.5 mM BAPTA; that with 2 μM [Ca2+]free was buffered by 0.5 mM diBrBAPTA; that with 55 μM [Ca2+]free was buffered by 0.5 mM nitrilotriacetic acid (NTA, Sigma 72559) (Dweck et al., 2005). [Ca2+]free in these solutions were verified using [Ca2+]-sensitive dye fluorimetry. The luminal solution with 300 μM [Ca2+]free was buffered by 1.5 mM Na2ATP according to Max Chelator freeware; and that with 600 μM [Ca2+]free was made using the activity coefficient of CaCl2 as described in Vais et al., 2010a. In the experiments involving MgATP to energize the SERCA, we used a solution containing 140 mM KCl, 10 mM K-HEPES, 0.5 mM K-BAPTA, 60 μM CaCl2, 1 mM MgATP, pH 7.3. Using the online Webmaxc Extended software, we calculated that our solution at 25°C has 0.30 mM free Mg2+ (with 73 nM Ca2+free, 0.30 mM ATP4–, and 0.42 mM free BAPTA).
The nuclear patch-clamp experiments in various patch-clamp configurations (on-nuc, cyto-out and lum-out) using DT40-r3 cells were acquired over an extensive period. To ensure the behaviors of these cells were consistent, we regularly used cells, cultured in identical conditions and at most one day apart from data-generating cells, to perform control experiments in which nuclei were patched in on-nuc or cyto-out configurations under optimal stimulatory conditions (with 10 μM InsP3, 2 μM [Ca2+]i and 0.5 mM ATP4- on the cytoplasmic side of the outer nuclear membrane). Our experience suggested that most newly-thawed DT40-r3 cells were consistent after culturing for 5 days. If the mean channel Po of a batch of control cells cultured for any time beyond day five was found to be significantly lower than that of previous control cells, that batch was terminated immediately and a new batch of cells was thawed out for new experiments.
InsP3R channel-current traces under constant or ramping applied potential (Vapp) were acquired at room temperature (RT) as described (Mak et al., 2007), digitized at 5 kHz, anti-aliasing filtered at 1 kHz. All Vapp were measured relative to the reference bath electrode regardless of the patch-clamp configuration used. InsP3R channel gating characteristics—number of active channels observed (NA) and open probability (Po)—were derived from current traces using semi-automatic QuB (Qin et al., 2000) and fully-automatic (Bruno et al., 2013) software and manually using IGOR Pro software (Wavemetrics). Only current traces long enough for NA to be determined with >99% confidence (Vais et al., 2010b) were used for statistical analysis.
Ca2+-dependent affinity-enrichment mass spectrometry
Obtaining samples of enriched peripheral ER-luminal proteins from bovine hepatocytes
Request a detailed protocolBovine liver was procured from three cows within three hours of slaughter, cut into large pieces of ~200 g each, rinsed with ice-cold PBS and flash frozen in –80°C freezer within one hr of procurement to be used later. The following protocol was used for processing 200 g of bovine liver. Quantities of reagents used were scaled according to amount of extracted proteins required. Bovine liver was thawed in ice-cold water and diced into small pieces of 0.8 cm3 (~0.5 g). 10 g of cut liver pieces and 19 ml of ice-cold DPBS with Mg2+ and Ca2+ (Corning cat # 21–030 CM) were put into each of twenty Stomacher 80 strainer bags (Seward cat # BA6040/STR) and processed individually in a Stomacher 80 Biomaster (Seward cat # 0080/000/AJ) at highest setting for 75 s to release intact hepatocytes. Cell suspension was strained through the strainer bags and collected (~500 ml). 250 ml of ACK lysing buffer (Quality Biological cat. # 118-156-101) at RT was mixed into the cell suspension to specifically lyse red blood cells. The process was terminated after 5 min by adding 500 ml DMEM (Corning cat. # 10–013-CV) with 10% FBS followed with gentle shaking. Hepatocyte suspension was centrifuged at 9,600 g for 18 min and the supernatant was discarded. Hepatocytes were rinsed twice by resuspending cells in 500 ml HBSS, centrifuging at 9,600 g for 18 min, and discarding the supernatant.
Hepatocytes were resuspended in 150 ml of homogenizing solution containing 150 mM KCl, 1 mM MgCl2, 1 mM CaCl2, 20 mM Tris HCl (pH 7.5), 400 μM phenylmethane sulfonyl fluoride (PMSF), and seven cOmplete protease inhibitor cocktail tablets (Roche cat. # 11697498001). Debris in cell suspension was removed with cell strainer. The hepatocytes were homogenized with nitrogen cavitation in an ice-cold large cell disruption vessel (Parr Instrument, Moline Il, model # 4635) using pressure of 1000 p.s.i. with constant stirring for 20 min. Cell homogenate was centrifuged at 3,300 g for 15 min to pellet unbroken cells and nuclei. The supernatant was centrifuged at 9,600 g for 15 min to pellet cell debris and mitochondria, and at 105,000 g for 15 min to pellet a crude microsomal fraction. The pellet was resuspended into 40 ml of 1.38 M sucrose solution, placed under a step gradient of 1.0 and 0.86 M sucrose and centrifuged at 300,000 g for 75 min. The smooth and rough ER fractions below the interface between 1.38 M and 1.0 M sucrose solution layers were collected and placed on ice.
To remove ribosomes from the rough ER, ice-cold sodium pyrophosphate (NaPPi)-imidazole HCl (NaPPi-I) solution containing 5 mM NaPPi and 3 mM imidazole-HCl, pH 7.4 was added dropwise to the collected ER fractions with continuous stirring on ice to the final volume of 100 ml. After a further 15 min of stirring, the mixture was centrifuged at 105,000 g for 37 min to re-pellet the microsomes. After discarding the supernatant, the ER microsome pellet was resuspended in 45 ml of sucrose-NaPPi-I solution containing 0.25 M sucrose, 5 mM NaPPi, and 3 mM imidazole HCl, pH 7.4; centrifuged again at 105,000 g for 37 min; and the supernatant was discarded.
The smooth ER microsome pellet was resuspended with vigorous vortexing in 8 ml of low-Ca2+ K+ with protease inhibitor (LCaK-PI) solution containing 150 mM KCl, 0.5 mM EGTA, 0.05% Tween-20, 25 mM Tris HCl (pH 7.5), 400 μM PMSF, one cOmplete protease inhibitor cocktail mini-tablet (Roche cat. #11836170001). The microsome suspension was processed with nitrogen cavitation twice using an ice-cold small cell disruption vessel (Parr Instrument, Moline Il, model # 4639) under 2200 p.s.i. with constant stirring for 20 min each cavitation. The homogenate was centrifuged at 105,000 g for 60 min to pellet the broken ER membrane. The supernatant was collected carefully without disturbing the ER membrane pellet so it contained only peripheral proteins released from the ER lumen in the presence of low [Ca2+]free (buffered by 0.5 mM EGTA in the LCaK-PI solution). Total protein concentration in the hepatocyte peripheral ER luminal protein (HPERLP) sample was determined using Bradford protein assay (~1.4–3.0 mg/ml). The HPERLP sample was aliquoted and stored in –80°C for future use.
Magnetic-bead pull down of peripheral proteins in the ER lumen that specifically interact with the luminal region of the InsP3R
Request a detailed protocolBased on the pL2 sequence in the L2 region of the InsP3R that is highly conserved among the three InsP3R isoforms (Figure 5B), peptides with a modified sequence (mpL2: K-Ahx-GNRGTFIRGYRAMVMDME) were synthesized for pull-down experiments. The Lys residue in pL2 was replaced with Arg (underlined) so that the mpL2 peptides could be coupled to magnetic beads through the only Lys (in italics) at the N-terminus. The unnatural 6-aminohexanoate residue (Ahx) was added to reduce possible steric hindrance that may interfere with the interaction between the peptide and ER luminal proteins. For control, peptides with a scrambled modified sequence (smpL2: K-Ahx-RDYRGMRMIMGETFNVGA) were also synthesized. Instructions of the manufacturer were followed to covalently couple the mpL2 and smpL2 peptides to NHS-activated magnetic beads (Pierce cat. # 88826) through the stable covalent link formed by reaction between the primary amine group of the N-terminal Lys of the peptides and the N-hydroxysuccinimide ester group on the magnetic beads. Peptide-coupled beads were stored (10 mg/ml) in storage buffer (150 mM NaCl, 25 mM Tris, pH 7.4 with 0.05% Tween-20% and 0.05% sodium azide) at 4°C.
A total of six pull-down procedures were performed in the cold with all apparatus and reagents at 4°C: one procedure using mpL2 peptide-coupled magnetic beads and one control procedure using smpL2 peptide-coupled magnetic beads for each of the three HPERLP samples from individual cows. The same protocol described below was used for each of the six procedures. To obtain sufficient protein for mass spectrometry, eight MACS separation columns (MS columns, Miltenyi Biotec cat. # 130-042-201) were used in each procedure. The MS columns were placed on the OctoMACS separator (Miltenyi Biotec cat. # 130-042-109) mounted on the MACS Multistand (Miltenyi Biotec cat. #130-042-303). To prime the columns, 250 μl of high-Ca2+ K+ (HCaK) solution containing 150 mM KCl, 1% NP–40 detergent (Thermo scientific cat. # 85124), 0.8 mM CaCl2, 25 mM Tris HCl (pH 7.5) was added to each. Effluent from the columns was discarded. 320 μl of peptide-coupled magnetic beads were resuspended in storage buffer, rinsed twice with HCaK solution, and resuspended with 290 μl of HCaK solution. 35 μl of the peptide-coupled magnetic bead suspension was added to each of the MS columns. Effluent was examined for presence of magnetic beads. If beads were detected, effluent was returned to the column till no beads were detected. Each column with magnetic beads were washed with 80 μl of HCaK solution and effluent was discarded. 360 μl of the HPERLP sample was thawed and HCaK solution and 1 M CaCl2 standard solution were added to adjust the total protein concentration in the final HCaK-HPERLP mixture to 1.25 mg/ml, and [CaCl2] to 800 μM ([Ca2+]free = 432 μM). 40 μl of the HCaK-HPERLP mixture was added to each column, followed by 80 μl of HCaK-PI solution—HCaK solution with additional 400 μM PMSF and 1% Halt protease inhibitor cocktail (Thermo Fisher Cat. # 78430). The magnetic beads in each column were rinsed once with 2 ml of HCaK-PI solution, and thrice with 2 ml of HCaK solution. Effluent was discarded. 200 μl of low-Ca2+ eluding (LCaE) solution with 150 mM KCl, 1% NP–40 detergent, 0.5 mM EGTA, 25 mM Tris HCl (pH 7.5) was added to each column. The eluate from all the columns was collected and frozen at –80°C.
Loading samples into mass spectrometer
Request a detailed protocolLow-Ca2+ eluate proteins from above were precipitated with 5 volumes of acetone held overnight at –20°C, decanted then solubilized in 20 µL of 1 × reducing NuPAGE LDS (Thermo Fisher Scientific) and run into a precast 10% Bis-Tris SDS-PAGE (Thermo Fisher Scientific) for 1.6 cm. After fixing overnight (25% ethanol, 7% acetic acid) the gel was stained with colloidal Coomassie blue dye. Each sample was excised from the gel in 4 (2 × 9 mm) slices and each cut into (1 mm)3 cubes. The gel pieces were destained in a solution containing 50% methanol and 1.25% acetic acid, reduced with 5 mM DTT (Thermo Fisher Scientific), and alkylated with 40 mM IAA (Sigma-Aldrich). The gel pieces were washed with 20 mM ammonium bicarbonate (Sigma-Aldrich) and dehydrated with acetonitrile (Fisher Scientific) twice. Sequencing-grade trypsin (Promega) (5 ng/µL in 20 mM ammonium bicarbonate) was added to the dehydrated-gel pieces and proteolysis was allowed to proceed overnight at 37°C. Peptides were extracted with 0.3% TFA (Fisher Scientific), followed by 50% acetonitrile. The volume of the combined extracts was reduced by vacuum centrifugation and 25% of the extracted peptides were analyzed per LC-MS/MS run (Glisovic-Aplenc et al., 2017).
LC-MS/MS mass spectrometry
Request a detailed protocolTryptic digests were analyzed by LC-MS/MS on a hybrid LTQ Orbitrap Elite mass spectrometer (Thermofisher Scientific San Jose, CA) coupled with a nanoLC Ultra (Eksigent). Peptides were separated by reverse phase (RP)-HPLC on a nanocapillary column, 75 μm id ×15 cm Reprosil-pur 3 μm, 120A (Dr. Maisch, Germany) in a Nanoflex chip system (Eksigent). Mobile phase A consisted of 1% methanol (Fisher)/0.1% formic acid (Thermo) and mobile phase B of 1% methanol/0.1% formic acid/80% acetonitrile. Peptides were eluted into the mass spectrometer at 300 nL/min with each RP-LC run comprising a 90 min gradient from 10% to 25% B in 65 min, 25–40% B in 25 min. The mass spectrometer was set to repetitively scan m/z from 300 to 1800 (R = 240,000 for LTQ-Orbitrap Elite) followed by data-dependent MS/MS scans on the twenty most abundant ions, with a minimum signal of 1500, dynamic exclusion with a repeat count of 1, repeat duration of 30 s, exclusion size of 500 and duration of 60 s, isolation width of 2.0, normalized collision energy of 33, and waveform injection and dynamic exclusion enabled. FTMS full scan AGC target value was 1e6, while MSn AGC was 1e4, respectively. FTMS full scan maximum fill time was 500 ms, while ion trap MSn fill time was 50 ms; microscans were set at one. FT preview mode; charge state screening, and monoisotopic precursor selection were all enabled with rejection of unassigned and 1+ charge states.
Sequence database search
Request a detailed protocolRaw MS files were processed using MaxQuant, version 1.6.1.0 for identification of proteins. The peptide MS/MS spectra were searched against the UniProtKB/Swiss-Prot Bovine Reference Proteome database, UP000009136 (retrieved on 12 July, 2018), comprising 24,333 entries including isoforms. Fragment ion tolerance was set to 0.5 Da, with full tryptic specificity required and a maximum of two missed tryptic cleavage sites. Precursor ion tolerance was seven ppm. Oxidation of methionine, acetylation of the protein N-terminus and conversion of glutamine to pyroglutamic acid were used as variable modifications. Carbamidomethylation of cysteine was set as a fixed modification. The minimal length required for a peptide was seven amino acids. Target-decoy approach was used to control false discovery rate (FDR). A maximum FDR of 1% at both the peptide and the protein level was allowed. If no unique peptide sequence to a single database entry was identified, the resulting protein identification was reported as an indistinguishable ‘protein group’. Protein groups containing matches to decoy database or contaminant proteins were discarded. The MaxQuant match-between-runs feature was enabled.
Statistical analysis of mass spectrometry output
Request a detailed protocolWe modeled the MS/MS spectral counts for each protein, sample pair using a hierarchical Poisson log-linear model. Our Bayesian method helped circumvent some of the problems that arise with small sample sizes by borrowing strength across proteins to better estimate the parameters in the model. We performed inference to determine the proteins that preferentially bound to the bait peptide found in InsP3R compared to the scrambled, control peptide using the false sign rate paradigm (Stephens, 2017).
Let be the number of observed MS/MS spectra for protein from cow in sample , where tt is 0 if the bait molecule was the scrambled peptide and one if the bait molecule was the modified InsP3R L2, that is a treated sample. In these data, and p=486p=486. For a point mass at 0, we model the data as follows:
and set . We added a pseudo count of 1 spectral count to each data point to avoid taking the log of 0. Note that adding a pseudo count only makes it more challenging to identify differences between the treatment and control conditions, and therefore leads to conservative inference. The above model also helped mitigate latent confounding variables and sources of over-dispersion by explicitly accounting for between-cow variation.
The goal was to estimate and perform inference on the treatment effect for each protein , where we were interested in identifying proteins with because these were indicative of proteins that were comparatively enriched in the treated, experimental samples. The local false sign rate for each protein is defined as the posterior probability that protein g did not preferentially bind to the InsP3R peptide:
The local false sign rates were computed by sampling from the posterior using Markov Chain Monte Carlo. A low LFSRG value indicates that the posterior probability of incorrectly identifying a protein as being enriched in the experimental samples is small. A threshold of LFSRG ≤ 0.2 (corresponding to a global false discovery rate of 5%) was applied to identify proteins with strong preference to bind to the L2 region of the InsP3R.
Confocal microscopy
Request a detailed protocolImages were collected on a Leica TCS SP8 X system using a 100x/1.4 NA PL APO CS2 objective. Annexin A1 was labeled with rabbit anti-Annexin A1 pAb (Proteintech, 21990–1-AP) and anti-rabbit AlexaFluor568 conjugated pAb (Invitrogen, A11011) was excited using a continuously tunable white light laser set to 568 nm to detect fluorescence emission between 600–700 nm. Calnexin was labeled with mouse anti-Calnexin mAb (Chemicon, MAB3126) and anti-mouse AlexaFluor488 conjugated pAb (Invitrogen, A11001) excited at 488 nm to detect fluorescence emission between 510–550 nm. DAPI was present in the mounting medium used to prepare the slides, excited at 408 nm to detect fluorescence emission between 430–470 nm.
Capture ELISA to monitor secretion of ANXA1 from HEKtsA201 cells
Sample preparation
Request a detailed protocolHEKtsA201 cells were seeded at 2 × 106 cells/10 cm tissue culture dish in 10 ml of 5% FBS/DMEM with 1 × Anti Anti, and grown at 37°C in 5% CO2 for 72 hr. Media in the dishes was collected, filtered through a 0.22 µm pore syringe filter, and concentrated 8-fold using Amicon Ultra-4 centrifugal filter devices (3 kDa MW-cutoff) as described in the manufacturer’s protocol. The cells in each dish were detached with Versene (5.4 mM EDTA) solution, pelleted by centrifugation at 1000 RPM for 5 min at 4°C, rinsed in 10 ml of 1 × DPBS, pelleted, and re-suspended in 1.5 ml of cell lysis buffer (50 mM Tris-HCL, 150 mM NaCl, 0.5 mM EGTA-NaOH, 0.3 mM CaCl2, and 0.2% w/v n-dodecyl β-d-maltoside) supplemented with 1 mM PMSF and Protease Inhibitor Cocktail (Roche). Lysates were incubated for 15 min on ice, centrifuged at 14,000 RPM for 10 min at 4°C to pellet genetic material released from nuclei. Supernatants were collected. Total [protein] was determined using the Pierce BCA Protein Assay kit (Thermo Fisher cat. # 23227).
Capture ELISA
Request a detailed protocolA high-binding, white, 96-well microtiter plate (Thermo, 7572) was coated with 100 µl/well of rabbit α-ANXA1 antibody (Proteintech, 21990–1-AP) diluted 1:500; or rabbit α-β actin antibody (Cell Signaling Technologies, 7881S) diluted 1:100 in carbonate capture buffer (6 mM Na2CO3; 44 mM NaHCO3; pH 9.6). Plates were incubated overnight at 4°C. The next day, the capture antibody solution was discarded, wells were rinsed 3 × with 200 µl of wash solution (50 mM Tris, 0.14 M NaCl, 0.05% Tween 20, pH 8.0), and 200 µl of blocking solution (50 mM Tris, 0.14 M NaCl, 1% BSA, pH 8.0) was added to each well and incubated for 30 min at RT. The wells were rinsed 3 × again as described before. 100 µl of each concentrated cell-culture media (supernatant) or cell lysate sample were added. Five-fold serial dilutions were made of concentrated supernatants (neat, 1:5, 1:25, 1:125 in cell culture media) and cell lysates (0.5, 0.1, 0.02, 0.004, 0.0008 mg/mL in cell lysis buffer) in six replicates. Wells containing cell-culture media or cell lysis buffer only were made in triplicate as negative controls. The plate was incubated overnight at 4°C. The next day, samples in the wells were discarded, and the wells rinsed 3×. 100 µl of primary mouse α-ANXA1 antibody (ECM Biosciences, AM0211) diluted 1:1000; or mouse α-pan actin antibody (Cell Signaling Technologies, 7881S) diluted 1:100 in antibody diluent (50 mM Tris, 0.14 M NaCl, 1% BSA, 0.05% Tween 20, pH 8.0) was added to the appropriate wells and incubated for 1 hr at RT. Contents in the wells were again discarded and the wells rinsed 3×. 100 µL of secondary goat α-mouse IgG-HRP antibody (Cell Signaling Technologies, 7074S) diluted 1:2000 in antibody diluent was added to each well, and incubated for 1 hr at RT. Again, contents in the wells were discarded and the wells rinsed 3×. 100 µL of PICO chemiluminescent HRP substrate (Pierce) was added to each well and incubated for 5 min at RT. Chemiluminescence was measured in a Cytation five plate reader (BioTek).
InsP3R-mediated intracellular Ca2+ release in HEKtsA201 cells expressing different levels of ANXA1
Acute knock-down of ANXA1 expression in HEKtsA201 cells by siRNA transfection
Request a detailed protocolWe performed knock-down experiments by transfecting human HEKtsA201 cells with human ANXA1 siRNA. For comparison, two kinds of controls were performed: HEKtsA201 cells were either transfected with non-targeting (N-T) siRNA or not transfected at all. Four pairs of controls and experiments were done: two pairs were experiments using ANXA1 siRNA-transfected cells versus controls using N-T siRNA-transfected cells, the other two were experiments using ANXA1 siRNA-transfected cells versus controls using non-transfected cells.
Following the siRNA transfection protocol from Dharmacon (Lafayette, CO), human ANXA1 siRNA (Dharmacon cat. # M-011161-01-0005) and N-T siRNA (Dharmacon cat. # D-001206-13-05) were suspended in 250 μl of 1 × siRNA buffer (50 μl of 5 × siRNA buffer (Dharmacon cat. # B-002000-UB-100) in 200 μl RNase-free water) to a final siRNA concentration of 20 μM, aliquoted and stored at –20°C. For a pair of control and experiment, 10 ml of HEKtsA201 cell suspension with density of ~0.26 × 106 cells/ml were plated into each of four 10 cm culture dishes (two for the experiment and two for the control) and incubated overnight (~18 hr) at 37°C. To transfect two 10 cm dishes of HEKtsA201 cells, 30 μl of 20 μM siRNA (ANXA1 or N-T) was thawed and diluted with 90 μl of RNase-free water. 3.9 ml of Opti-MEM (Gibco cat. # 31985–070) was added to the siRNA, mixed by gentle pipetting. The siRNA mixture was incubated for 7 min. For a non-transfected control, 4 ml of Opti-MEM was used. 160 μl of transfection reagent (Dharmacon cat. # T-2001–02) was diluted with Opti-MEM to a final volume of 8 ml, mixed by gentle pipetting. The resulting transfection solution was incubated for 7 min. 4 ml of transfection solution was added to the 4 ml of siRNA mixture (for experiment ANXA1 or control N-T siRNA transfection) or 4 ml of Opti-MEM solution (for non-transfection control). The resulting mixtures were incubated for another 25 min. Each of the mixtures was then diluted with 32 ml of antibiotic-free complete medium (DMEM (Corning cat. # 10–013-CV) with 10% FBS (HyClone cat. # SH30071.03) to give 40 ml of transfection medium.
Culture medium was removed from each of the four dishes of HEKtsA201 cells that had been incubated overnight. 20 ml of ANXA1 siRNA transfection medium was added to each of two dishes for the experiment; and 20 ml of N-T siRNA transfection medium or non-transfection medium was added to each of two dishes for the control. The cells in transfection medium were incubated for 6 hr at 37°C. After the incubation, the transfection medium was replaced with 20 ml of regular HEKtsA201 cell medium for each of the four dishes of cells. Cells were incubated at 37°C for an additional 42 hr before being used for measurements of intracellular Ca2+ release.
Expression levels of ANXA1 in HEKtsA201 cells were probed in Western blots using anti-ANXA1 antibody (Proteintech cat. # 21990–1-AP, 1:1000 dilution), stripped and re-probed with anti-β-actin antibody (Cell Signalling cat. # 8H10D10, 1:1000 dilution).
Spectrofluorimetry of intracellular Ca2+ release stimulated by extracellular agonist
Request a detailed protocolThe same protocol was used to perform fluorimetry for experiment and control HEKtsA201 cells. After incubation,~10–20 × 106 cells (ANXA1 siRNA transfected, N-T siRNA transfected or non-transfected) were in each 10 cm culture dish. To collect the attached cells, the HEKtsA201 medium was removed, the cells were rinsed once with 10 ml of Ca2+-free DPBS (Corning cat. # 21–031 CM) at RT, incubated in 5 ml of Versene solution (Gibco cat. # 15040–066) for 20 min to detach, dispersed by gently pipetting the cell suspension, and the cell density was determined using a hemocytometer. Four million cells were used to quantify the expression level of ANXA1 in the HEKtsA201 cells by Western blotting. The remaining cells were centrifuged at 350 g for 3 min. The supernatant was discarded, and the cell pellet was resuspended in 10 ml of Fura-2 AM dye-loading solution (1 μM Fura-2 AM dye (Molecular Probes cat. # I-1225) and 0.01% pluronic F127 (Thermo Fisher cat. # P3000MP) in HEPES-buffered saline (HBS) containing 135 mM NaCl, 5.9 mM KCl, 1.2 mM MgCl2, 1.5 mM CaCl2, 11 mM glucose, and 11.6 mM Na-HEPES (pH 7.4). The cell suspension was kept in darkness with gentle shaking for 20 min at RT. The dye-loaded cells were then centrifuged at 350 g for 3 min. The supernatant was discarded, and the cell pellet was resuspended in 10 ml HBS. The cell suspension was again centrifuged at 350 g for 3 min. The supernatant was discarded, and the cell pellet was resuspended in HBS to a cell density of 3–4 × 106 cells/ml. These cells were kept in darkness. Each 10 cm dish of cells was sufficient for 4 to 7 assays. For proper control, dishes of ANXA1 siRNA-transfected cells and control cells were used alternately. Just before each assay, 0.75 ml of cell suspension was centrifuged in a 1.5 ml eppendorf tube at 400 g for 3 min. The supernatant was discarded and the cells were resuspended in 0.75 ml of HBS and transferred to a cuvette containing 0.75 ml of HBS and a 3–mm magnetic stirrer. The cuvette was transferred to the temperature-controlled (37°C) experimental compartment of a multi-wavelength-excitation dual-wavelength-emission high-speed spectrofluorometer (Delta RAM, Photon Technology International). Fluorescence at 340 nm excitation/515 nm emission and 380 nm excitation/515 nm emission for the Ca2+-bound and Ca2+-free Fura-2 species, respectively, were measured at 5 Hz. The ratio (R) of the fluorescence intensity excited by 340 nm versus 380 nm light was used as relative measurement of intracellular [Ca2+]free. After a stable baseline of R had been observed for 90 s, 15 μl of 10 mM carbachol solution was added to the cell suspension (final 10 μM carbachol) to stimulate sub-maximal InsP3R-mediated release of Ca2+ from the ER. R was further observed for another 120 s.
Imaging histamine-induced Ca2+ signals in HeLa cells expressing different levels of ANXA1
Request a detailed protocolHeLa cells were cultured on 15 cm tissue culture dishes in Dulbecco’s Modification of Eagle’s (DMEM Corning) supplemented with 10% fetal bovine serum (Hyclone) and maintained at 37°C in a humidified incubator gassed with 95% air and 5% CO2. Transfection with siRNA for either human ANXA1 siRNA or non-targeting siRNA control was performed as described for HEKtsA201 cells. ~ 3 × 105 cells were seeded on each 12 mm coverslip. At 48 hr post-transfection, cells were loaded with 2 µM Fura-2 AM for 15–20 min then incubated in 2 Ca Tyrode’s solution for 5–10 min at room temperature prior to imaging. Cells were imaged on a Nikon Ti system using a 20x/0.75 NA objective for fluorescence at 340 nm excitation/515 nm emission (Ca2+-bound Fura2), and 380 nm excitation/515 nm emission (Ca2+-free Fura2). Coverslips were perfused with 2 Ca Tyrode’s solution for 30 s, 10 or 100 µM histamine in 2 Ca Tyrode’s solution for 360 s or 120 s respectively, followed by a washout with 2 Ca Tyrode’s solution for 90 s. 100 ms exposure images for each wavelength were collected every 2 s. For analysis of intracellular Ca2+-signals, cells were mass-selected using a binary mask and the Time Series Analyzer v3 plugin in ImageJ (NIH). The 340 nm/380 nm (Rfura2) fluorescence ratio for each time point was measured for every cell in the field of view and the normalized signal (R/R0) was calculated by dividing Rfura2 for each time point by the mean Rfura2 during the first 30 s of each experiment. A series of logic tests were applied to data to identify signaling cells and separate those cells into oscillating and non-oscillating groups. To exclude cells that did not begin and end at baseline Ca2+ levels, only cells with R/R0 values between 1.25–0.75 during the first 30 s and R/R0 values less than 1.5 during the last 30 s of the final washout were selected. To exclude non-responding cells, only cells with maximal R/R0values ≥ 2.0 following histamine stimulation were selected. Cells with a coefficient of variation (%CV) value greater than 15% measured from the end of the initial Ca2+ signal to the end of the histamine stimulation were considered oscillating cells. Oscillating cells were qualitatively characterized as exhibiting either ‘periodic oscillation’ or ‘random spiking’ pattern.
Monitoring intracellular elementary Ca2+ release events (Ca2+ puffs) in HEK293 cells by total internal reflection microscopy
Cell culture and siRNA transfection
Request a detailed protocolWT HEK-293 cells were cultured on plastic 75 cm tissue culture flasks in Eagle’s Minimum Essential Medium (EMEM; ATCC #30–2003) supplemented with 10% fetal bovine serum (Omega Scientific #FB-11), and maintained at 37°C in a humidified incubator gassed with 95% air and 5% CO2. For transfection with siRNA, cells were collected using 0.25% Trypsin-EDTA (Gibco #25200–056) and grown on 60 mm culture dishes. When cells reached 80% confluence they were incubated with 15 nM ANXA1 siRNA or with 15 nM non-targeting CTL siRNA together with 15 µl of DharmaFECT transfection reagent (GE Healthcare) for 6 hr. In some experiments, cells were additionally incubated with 5 nM siGLO Red Transfection Indicator (Dharmacon #D-001630-02-05) to serve as a fluorescent tracer to visualize transfection efficiency. Following incubation, cells were harvested using 0.25% Trypsin-EDTA, pelleted by low speed centrifugation (~800 x g), resuspended in EMEM and distributed among poly-D-lysine coated (1 mg/ml; Sigma #P0899) 35 mm glass-bottom imaging dishes (MatTek #P35-1.5–14 C) where they were grown for 48 hr prior to imaging, at which time cells were ~50% confluent.
Immediately before imaging, cells were incubated with membrane-permeable esters of the fluorescent Ca2+ dye Cal-520/AM (5 µM; AAT Bioquest #21130) and the caged IP3 analogue ci-IP3/PM [D-2,3,-O-Isopropylidene-6-O-(2-nitro-4,5 dimethoxy) benzyl-myo-Inositol 1,4,5,-trisphosphate Hexakis (propionoxymethyl) ester] (1 µM; SiChem #cag-iso-2-145-10) for 1 hr at RT in a Ca2+-containing HEPES buffered salt solution (Ca2+-HBSS). Cells were then washed with Ca2+-HBSS and loaded for an additional hour with EGTA/AM (5 µM; ThermoFisher #E1219). Cal-520/AM, caged i-IP3/PM, and EGTA/AM were all solubilized with DMSO/20% pluronic F127 (ThermoFisher #P3000MP). Ca2+-HBSS contained (in mM) 135 NaCl, 5.4 KCl, 2 CaCl2, 1 MgCl2, 10 HEPES, and 10 glucose (pH = 7.4 at RT).
Ca2+ imaging
Request a detailed protocolTotal internal reflection fluorescence (TIRF) imaging of Ca2+ signals was accomplished using a home-built system, based around an Olympus IX50 microscope equipped with an Olympus 60X objective (NA 1.45). Using 488 nm laser fluorescence excitation and a 510 nm long pass emission filter, fluorescence images were captured with an Evolve EMCCD camera (Photometrics), utilizing 2 × 2 pixel binning for a final field of 128 × 128 pixels (one pixel = 0.53 µm) at a rate of ~125 frames s−1. To photo-release i-IP3, UV light from a xenon arc lamp was filtered through a 350–400 nm bandpass filter and introduced by a UV-reflecting dichroic in the light path to uniformly illuminate the field of view. The amount of i-IP3 released was controlled by varying the flash duration, set by an electronically controlled shutter (UniBlitz). All image data were streamed to computer memory using Metamorph v7.7 (Universal Imaging/Molecular Devices) and stored on hard disc for offline analysis.
Image analysis
Request a detailed protocolImage data in MetaMorph stk format were processed using Flika (Ellefsen et al., 2014), a freely available open-source image processing and analysis software written in the Python programming language (Ellefsen et al., 2019). Fluorescence records of 30 s and 10 s immediately following the UV flash were analyzed for the 50 ms and 150 ms flash durations, respectively; shorter records were analyzed for the 150 ms flash duration because of rapidly rising global Ca2+ levels which hamper measurement of local Ca2+ signals. Raw fluorescence records were first black-level subtracted and then processed to create a ratio image stack (F/F0), where the fluorescence intensity of each pixel in a given frame was replaced by that intensity (F) divided by the mean resting fluorescence intensity at that pixel averaged over 500 frames prior to photo-release of i-IP3 (F0). Next, a custom plug-in (‘detect puffs’) was applied for automated detection and analysis of local Ca2+ signals. All Ca2+ puffs identified by the algorithm were verified by visual inspection prior to further analysis. Measurement of peak puff amplitudes (ΔF/F0) and kinetics were performed by the algorithm on a 5 × 5 pixel region of interest centered over the centroid of each event, and were exported to EXCEL spreadsheets for further analysis. Additional analysis and graphing was performed in Microcal Origin v6.0 (OriginLab) and Igor 6 (WaveMetrics).
Quantification and statistical analyses
Request a detailed protocolAll measurements in this study: InsP3R channel open probabilities (Po), normalized probabilities of detection of InsP3R channel activity (Pd), normalized maximal change of fluorescence intensity ratio (ΔRmax) and normalized rate of change of fluorescence intensity (1/τ), number of Ca2+ puffs per second per imaging field and amplitudes of the Ca2+ puffs (ΔF/F0), performed under various experimental conditions were compared using unpaired t-test. For data sets involved in multiple comparisons, p values were determined using the Bonferroni correction for multiple comparisons. Quantified western blot intensities from co-immunoprecipitation experiments were compared by paired t-test.
Data availability
All data generated and analyzed are included in the manuscript and supporting files.
References
-
The inositol trisphosphate/Calcium signaling pathway in health and diseasePhysiological Reviews 96:1261–1296.https://doi.org/10.1152/physrev.00006.2016
-
Annexin A1 localization and its relevance to CancerClinical Science 130:205–220.https://doi.org/10.1042/CS20150415
-
A mediator of cell surface-specific plasmin generationAnnals of the New York Academy of Sciences 947:143–155.
-
A reassessment of the effects of luminal [Ca2+] on inositol 1,4,5-trisphosphate-induced Ca2+ release from internal storesThe Journal of Biological Chemistry 278:39503–39508.https://doi.org/10.1074/jbc.M305823200
-
Proteomic and bioinformatic characterization of the biogenesis and function of melanosomesJournal of Proteome Research 5:3135–3144.https://doi.org/10.1021/pr060363j
-
Calcium, a signaling molecule in the endoplasmic reticulum?Trends in Biochemical Sciences 25:307–311.https://doi.org/10.1016/S0968-0004(00)01588-7
-
Expanding the range of free calcium regulation in biological solutionsAnalytical Biochemistry 347:303–315.https://doi.org/10.1016/j.ab.2005.09.025
-
Applications of FLIKA, a Python-based image processing and analysis platform, for studying local events of cellular calcium signalingBiochimica Et Biophysica Acta (BBA) - Molecular Cell Research 1866:1171–1179.https://doi.org/10.1016/j.bbamcr.2018.11.012
-
Macrophage surface expression of annexins I and II in the phagocytosis of apoptotic lymphocytesMolecular Biology of the Cell 15:2863–2872.https://doi.org/10.1091/mbc.e03-09-0670
-
Inositol trisphosphate receptor Ca2+ release channelsPhysiological Reviews 87:593–658.https://doi.org/10.1152/physrev.00035.2006
-
Annexins: from structure to functionPhysiological Reviews 82:331–371.https://doi.org/10.1152/physrev.00030.2001
-
Suppression of MIP-2 or IL-8 production by annexins A1 and A4 during coculturing of macrophages with late apoptotic human peripheral blood neutrophilsBiochimica Et Biophysica Acta (BBA) - Molecular Basis of Disease 1822:204–211.https://doi.org/10.1016/j.bbadis.2011.10.013
-
Endogenous signalling pathways and caged IP3 evoke Ca2+ puffs at the same abundant immobile intracellular sitesJournal of Cell Science 130:3728–3739.https://doi.org/10.1242/jcs.208520
-
The calcium pump of the liver nuclear membrane is identical to that of endoplasmic reticulumThe Journal of Biological Chemistry 267:11548–11552.
-
Annexin A1-containing extracellular vesicles and polymeric nanoparticles promote epithelial wound repairJournal of Clinical Investigation 125:1215–1227.https://doi.org/10.1172/JCI76693
-
Spatial-temporal patterning of Ca2+ signals by the subcellular distribution of IP3 and IP3 receptorsSeminars in Cell & Developmental Biology 94:3–10.https://doi.org/10.1016/j.semcdb.2019.01.012
-
ATP regulation of recombinant type 3 inositol 1,4,5-trisphosphate receptor gatingJournal of General Physiology 117:447–456.https://doi.org/10.1085/jgp.117.5.447
-
BookNuclear patch clamp electrophysiology of inositol trisphosphate receptor Ca2+ release channelIn: Foskett J, Putney J. W, editors. Calcium Signaling (Second). Boca Raton: CRC Press. pp. 203–229.
-
Isolating nuclei from cultured cells for patch-clamp electrophysiology of intracellular Ca2+ channelsCold Spring Harbor Protocols 2013:880–884.https://doi.org/10.1101/pdb.prot073056
-
Patch-clamp electrophysiology of intracellular Ca2+ channelsCold Spring Harbor Protocols 2013:880–884.https://doi.org/10.1101/pdb.top066217
-
Nuclear patch-clamp electrophysiology of Ca2+ channelsCold Spring Harbor Protocols 2013:885–891.https://doi.org/10.1101/pdb.prot073064
-
Endoplasmic-reticulum calcium depletion and diseaseCold Spring Harbor Perspectives in Biology 3:a004317.https://doi.org/10.1101/cshperspect.a004317
-
Co-expression in vertebrate tissues and cell lines of multiple inositol 1,4,5-trisphosphate (InsP3) receptors with distinct affinities for InsP3The Journal of Biological Chemistry 269:28613–28619.
-
Structural basis for the regulation of inositol trisphosphate receptors by Ca2+ and IP3Nature Structural & Molecular Biology 25:660–668.https://doi.org/10.1038/s41594-018-0089-6
-
Annexins: the problem of assessing the biological role for a gene family of multifunctional calcium- and phospholipid-binding proteinsBiochimica Et Biophysica Acta (BBA) - Reviews on Biomembranes 1197:63–93.https://doi.org/10.1016/0304-4157(94)90019-1
-
Dexamethasone-induced translocation of lipocortin (annexin) 1 to the cell membrane of U-937 cellsBritish Journal of Pharmacology 112:347–348.https://doi.org/10.1111/j.1476-5381.1994.tb13075.x
-
False discovery rates: a new dealBiostatistics 18:275–294.https://doi.org/10.1093/biostatistics/kxw041
-
Imaging intraorganellar Ca2+ at subcellular resolution using CEPIANature Communications 5:4153.https://doi.org/10.1038/ncomms5153
-
Unitary Ca2+ current through recombinant type 3 InsP3 receptor channels under physiological ionic conditionsJournal of General Physiology 136:687–700.https://doi.org/10.1085/jgp.201010513
-
Permeant calcium ion feed-through regulation of single inositol 1,4,5-trisphosphate receptor channel gatingJournal of General Physiology 140:697–716.https://doi.org/10.1085/jgp.201210804
-
Calcium binding proteinsAdvances in Experimental Medicine and Biology 740:461–482.https://doi.org/10.1007/978-94-007-2888-2_19
-
Intracellular organelles in the Saga of Ca2+ homeostasis: different molecules for different purposes?Cellular and Molecular Life Sciences 69:1077–1104.https://doi.org/10.1007/s00018-011-0845-9
Article and author information
Author details
Funding
National Institutes of Health (R37GM56328)
- J Kevin Foskett
National Institutes of Health (R01GM114042)
- Don-On Daniel Mak
National Institutes of Health (GM048071)
- Ian Parker
The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.
Acknowledgements
This work was supported by NIH grants R37 GM 56328 (JKF), R01 GM 114042 (D-ODM) and GM 048071 (IP).
Copyright
© 2020, Vais et al.
This article is distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use and redistribution provided that the original author and source are credited.
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